INHIBITION OF PRIMARY COLONIZERS BY
MARINE SURFACE-ASSOCIATED
BACTERIA
By
Vipra Nandani KUMAR
A Thesis Submitted in Partial Fulfilment of the
Requirements for the Degree of
Master in Science in Biology
School of Biological, Chemical and Environmental Sciences
Faculty of Science and Technology
The University of the South Pacific
2009
i
Abstract
Surfaces immersed in seawater rapidly accumulate a complex biofouling community,
of which bacteria and diatoms are among the first colonisers. However marine
organisms have evolved several defence mechanisms and it has been suggested that
green algae of the genus Ulva rely on microbial defence. The antibacterial properties
of epiphytic bacteria are well established, but relatively little is known about their
anti-diatom properties. In this study the hypothesis that surface-associated bacteria
from tropical Ulva species have anti-fouling characteristics that may have a role in
preventing surface fouling on the algae was investigated. Bacterial isolates from the
surface of Ulva growing in tropical waters were obtained and tested for antibacterial
and anti-diatom properties. It was found that 60% of the isolates expressed some
inhibitory action against the remaining bacteria isolated in the study and 80%
inhibited growth of the diatom Cylindrotheca fusiformis. Most effective bacteria were
members of the Pseudoalteromonas genus. Also showing inhibitory properties were
members of the genus Bacillus, Vibrio and Shewanella. Since Pseudoalteromonas
spp. and the Roseobacter clade are model surface-associated bacteria, both groups
were screened for anti-diatom property. Results showed that anti-diatom activity was
present in 100% and 44% of tested Pseudoalteromonas and Roseobacter strains
respectively. In order to better comprehend the anti-diatom property of marine
surface-associated bacteria, a transposon mutant library of Pseudoalteromonas
tunicata was generated and screened for mutants lacking in anti-diatom activity.
Genetic analysis of transposon insertion sites into the P. tunicata genome was then
used to identify loci linked with anti-diatom activity. Genes identified in this way
include a cation/multidrug efflux pump, a beta-hexosaminidase protein, a RTX toxin-
like gene and a member of the HemeO protein family. A hypothetical model for the
regulation of anti-diatom activity in P. tunicata was suggested and this will form the
basis of future studies that aim to identify the mechanism of anti-diatom activity in
bacteria, especially in P. tunicata. Additionally, the presence of epiphytic bacteria
engaged in antifouling activities on the surface of tropical Ulva sp. emphasizes the
prevalence of microbial-mediated defence systems which can be manipulated to find
solutions to current biofouling-associated problems.
ii
Acknowledgement
I extend my appreciation to the Faculty of Science and Technology of the University
of the South Pacific for awarding me with a Graduate Assistantship and funding this
research. Sincere thanks are also conveyed to the Centre for Marine Bio-Innovation,
University of New South Wales for collaborating in this research. To my supervisors,
Dr. Dhana Rao of University of the South Pacific, Dr. Suhelen Egan and Prof. Staffan
Kjelleberg of University of New South Wales, I am greatly honoured to have worked
under you. Your constant guidance and companionship has brought out the best in this
project. Please accept my utmost gratitude.
I owe much thanks to Ani, Francesco, Mel, Cathy and Flavia for going over various
procedures with me. Thanks to Torsten for expert advice with phylogenetics. Special
thanks go out to Richard and Preeti for their assistance with editing and proof-reading.
I am grateful also to the Division of Biology for assisting in having my isolates sent
over. To Debra, Anne, Jeyran, Neil, Nico and the 304 team, thanks for making
everyday at CMB so much fun. A hearty thanks to all relatives and friends for your
continuous love and support. Heartfelt thanks also to friends and elders of Rooty Hill
Sai Centre for having made me a part of their ‘Sai family’.
I offer my highest salute to my devoted and loving parents for ensuring the best of
everything for me. Thank you for your constant encouragement and endless support.
And to my most treasured brother and sister-in-law, I do not know how to thank you
enough. Thank you for looking after me and ensuring warm meals and a cosy bed. I
am deeply indebted to your immense love and understanding.
Finally, thank you to my most beloved Swami for being my inspiration and guide. I
humbly dedicate this thesis to you, dear Lord.
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i
Table of Contents
List of Acronyms
ATP adenosine triphosphate
BLAST Basic Local Alignment
Search Tool
bp base pairs
Da Dalton
DM non anti-diatom mutant
DNA deoxyribonucleic acid
dNTP deoxynucleotide
triphosphate
EDTA ethylene diamine
tetraacetic acid
EPS extracellular polymeric
substances
g grams
g gravitational force
hr hours
IMG Intergrated Microbial
Genomes
kb kilobases, 1000bp
kDa kilodaltons, 1000 Da
Km kanamycin
l litres
LB Luria Broth
m milli (10-3)
M molar
min minutes
mm millimetres
mol moles
n nano (10-9)
NCBI National Centre for
Biotechnology
Information
ORF open reading frame
p pico (10-12)
PCR polymerase chain
reaction
rRNA ribosomal ribonucleic
acid
SDS sodium dodecyl sulfate
sec seconds
Sm streptomycin
SmR streptomycin resistant
sp. species
TBE tris-boric acid-EDTA
buffer
TBT tributyl tin
v/v volume to volume
w/v weight to volume
� lambda
μ micro (10-6)
°C degrees Celsius
ii
List of Tables
Table 2.1: Antibacterial activity expressed by bacteria isolated from Ulva…………22
Table 2.2: Inhibition of C. fusiformis as expressed by bacteria isolated from Ulva…23
Table 2.3: 16S rRNA gene identification of bacteria isolated from Ulva……………24
Table 3.1: Restriction enzymes used for panhandle PCR……………………………38
List of Figures
Figure 1.1: The stages of colonisation of surfaces immersed in seawater………….....2
Figure 1.2: Stages of biofilm development…………………………………….….…..4
Figure 1.3: Schematic diagram of diatom structure and frustule terminology…….....12
Figure 3.1: Diatom growth inhibition by Pseudoalteromonas spp………………......40
Figure 3.2: Diatom growth inhibition by members of the Roseobacter clade..……...41
Figure 3.3: Anti-diatom activity of wild type P. tunicata and non-antidiatom
mutants (DM1, DM2, DM3 and DM4)………………………………….…...42
Figure 3.4: Growth curve of wild type and mutant strains of P. tunicata………........43
Figure 3.5: Agarose gel showing the results from a typical panhandle-PCR ….…….44
Figure 3.6: Genomic location of PTD2_12754, homologous to AcrB/AcrD/AcrF
family protein………………………………………………………………...45
Figure 3.7: Genomic location of PTD2_01386 and PTD2_01391, homologous to
beta-hexosaminidase and RTX toxin respectively…………………………. ..45
Figure 3.8: Genomic location of PTD2_02946, a HemeO protein family..………….46
Figure 4.1: Hypothetical model for the regulation of anti-diatom activity
in P. tunicata………………………………………………………………….57
Figure 8.1: Phylogenetic relationship of isolate U3 to bacteria on ARB
Project Database…………………………………………………...…………63
Figure 8.2: Phylogenetic relationship of isolate U4 to bacteria on ARB
Project Database………………………….…………………………...…...…64
Figure 8.3: Phylogenetic relationship of isolate U7 and U11 to bacteria on
ARB Project Database………………………………………………………..65
Figure 8.4: Phylogenetic relationship of isolate U8 to bacteria on ARB
Project Database……………………………………………..…………….…66
iii
Figure 8.5: Phylogenetic relationship of isolate U13 and U14 to bacteria on
ARB Project Database………………………………...………………….…..67
Figure 8.6: Phylogenetic relationship of isolate U15 to bacteria on ARB
Project Database…………………………………………………...…………68
Figure 9.1: P. tunicata genome sequence section showing the point of insertion
of Tn10 in DM1……………………………………………………..………..69
Figure 9.2: P. tunicata genome sequence section showing the point of insertion
of Tn10 in DM2…………………………………………………….…….…..71
Figure 9.3: P. tunicata genome sequence section showing the point of insertion
of Tn10 in DM3………………………………………………………………75
List of Appendices
Appendix I: Media and buffers 78
Appendix II:Primers 81
Appendix III: Phylogenetic relationship of algal isolates to bacteria on ARB Project
database 82
Appendix IV: Transposon insertion sites in the P. tunicata genome 88
iv
Abstract i
Chapter 1: Introduction 1
1.1 Biofouling in the marine environment 1
1.1.1 The process and its importance 1
1.1.2 The role of biofilms 2
1.1.3 Current biofouling control strategies and its impact on the marine ecosystem 6
1.1.4 Natural defence mechanisms against biofouling 6
1.2 Diatoms as marine surface colonisers 11
1.2.1 Diatom biology 11
1.2.2 Diatom adhesion, motility and extracellular polymeric substances 13
1.3 Aims of this study 14
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva 16
2.1 Introduction 16
2.2 Materials and methods 17
2.2.1 Isolation of epiphytic bacteria from Ulva 17
2.2.2 Bioassay against growth of bacteria 18
2.2.3 Bioassay against growth of diatoms 18
2.2.4 Identification of isolates with inhibitory properties 19
2.2.4.1 DNA extraction 19
2.2.4.2 Agarose gel electrophoresis 19
2.2.4.3 PCR amplification of 16S rRNA gene 20
2.2.4.4 DNA sequencing and sequence analysis 20
2.3 Results 21
2.3.1 Epiphytic bacteria isolated from Ulva 21
2.3.2 Production of extracellular antibacterial compounds 21
2.3.3 Growth inhibition of diatoms 22
2.3.4 Characterization of active bacterial strains 23
2.4 Discussion 27
2.4.1 Antibacterial activity of bacterial isolates 27
2.4.2 Anti-diatom activity of bacterial isolates 27
v
2.4.3 Identification of active bacterial strains 28
2.5 Conclusion 32
Chapter 3: Anti-diatom property of Pseudoalteromonas and Roseobacter
strains 33
3.1 Introduction 33
3.2 Materials and methods 34
3.2.1 Screening Pseudoalteromonas and Roseobacter strains for anti-diatom activity
34
3.2.2 Analysis of anti-diatom strategy of P. tunicata 35
3.2.2.1 Transposon mutagenesis 35
3.2.2.2 Screening for P. tunicata mutants lacking anti-diatom property 36
3.2.2.3 Growth rates of mutants 36
3.2.2.4 Genomic DNA extraction of non anti-diatom mutants 37
3.2.2.5 Generation of adaptor ligated DNA for panhandle PCR 37
3.2.2.6 Panhandle PCR 38
3.2.2.7 Sequencing 39
3.3 Results 39
3.3.1 Growth inhibition of diatoms 39
3.3.2 Mutants lacking in anti-diatom activity 42
3.3.3 Growth curve of wild type and mutants of P. tunicata 43
3.3.4 Panhandle PCR and DNA sequencing 43
3.3.5 Genotype characterization of the non anti-diatom mutants 44
3.3.5.1 DNA regions flanking the transposon insertion site in DM1 44
3.3.5.2 DNA regions flanking the transposon insertion site in DM2 45
3.3.5.3 DNA regions flanking the transposon insertion site in DM3 46
3.4 Discussion 46
3.4.1 Anti-diatom activity of Psedoalteromonas spp. and Roseobacter clade 46
3.4.2 Analysis of transposon insertion sites within the P. tunicata genome 48
3.5 Conclusion 53
vi
Chapter 4: General discussion 54
4.1 Antifouling properties of surface-associated bacteria 54
4.2 Modelling anti-diatom mechanism in P. tunicata 55
4.3 Future directions and implications 58
References 59
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 1
Chapter 1: Introduction
1.1 Biofouling in the marine environment
1.1.1 The process and its importance
Biofouling is the undesirable accumulation of microorganisms, plants and animals on
surfaces immersed in water. It is a dynamic process involving a sequence of
colonization events that lead to the formation of a mature fouling community.
Dobretsov et al., (2006) viewed the colonization of a substratum in aquatic systems as
a three-step process (Figure 1.1). The process involves (i) adsorption of dissolved
organic molecules to a newly submerged or otherwise uncolonised surface, (ii)
colonization of the surface by bacteria and microscopic eukaryotes (e.g., diatoms,
fungi, and other heterotrophic eukaryotes) and (iii) settlement and subsequent growth
of invertebrate larvae and algal spores.
Biofouling impacts on humans in a number of ways, perhaps most important are the
potential economic effects. Any industry that is reliant upon or linked to aquatic
environments must deal with the effects of biofouling (e.g., offshore oil and gas
sectors, fishing and aquaculture industries and the transport industry). Perhaps the
most common biofouling sites are ships hulls. A heavily fouled vessel suffers
increased drag and decreased manoeuvrability due to the roughness of the hull. This
has major economic implications, potentially resulting in a significant increase in fuel
costs. Biofouling may also lead eventually to corrosion of the hull that may reduce the
lifespan for the vessel. Other surfaces, in particular those exposed directly to water
(e.g., heat exchangers, ballast tanks, and propellers), may also be subject to biofouling
(Brizzolara, 2002). In addition, equipment used in fishing and fish farming (e.g., mesh
cages and trawls) are also likely to harbour fouling organisms.
Living surfaces in the marine environment are also prone to biofouling. Macroalgae
are particularly susceptible since they are sessile and often restricted to the photic
zone where conditions for fouling are optimal (de Nys et al., 1995).
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 2
Molecular fouling Micro-fouling
Settlement of bacteria and diatoms
Adsortpion of conditioning film
Macro-fouling
Settlement of macroalgae and invertebrate larvae
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Besides providing a large surface area for colonization, algae may also provide a
source of nutrients and shelter for epibionts. Biofouling on marine organisms can
have detrimental effects on the host such as loss of photosynthetic area, reduced
viability, and organism death (Holmstrom and Kjelleberg, 2000). Biofouling may
impair the ability of the host to exchange gases and nutrients. Toxins, digestive
enzymes and waste produced by the biofouling community may also cause physical
damage to the host (Felgenhaur et al., 1989).
1.1.2 The role of biofilms
Each of the three stages in the formation of a biofouling community is an important
pre-requisite for the establishment of subsequent layers. In particular the microfouling
stage (the second stage in Figure 1.1), which involves the formation of a microbial
biofilm, initiates colonization for higher organisms. Studies have found that the
bacterial component of marine biofilms are important for induction of larval
settlement in several groups including echinoderms (Johnson et al., 1991), cnidarians
(Negri et al., 2001), polychaetes (Unabia and Hadfield, 1999), gastropods (Rodriguez
et al., 1995) and crustaceans (Neal and Yule, 1994). Hence an understanding of
biofilm formation is essential for developing an overall understanding of the
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 3
biofouling process. Although biofilms are composed of both bacteria and diatoms, our
current general understanding of biofilm formation has been gained from bacterial
biofilms. Biofilms are multicellular associations, consisting of closely spaced cells
embedded in an extracellular matrix. The process of bacterial biofilm formation
involves cell attachment, microcolony formation, biofilm maturation and cell
dispersal (Figure 1.2).
The first stage in biofilm formation involves surface attachment. Upon encountering a
suitable surface, planktonic cells adhere to the conditioning film and establish a weak
interaction with the surface. This initial phase is referred to as “reversible attachment”
(Busscher et al., 1992). Adhesion is influenced by many factors including the
physico-chemical properties of the cell surface (e.g., cell surface hydrophobicity;
Bruinsma, 2001), genetic determinants of the cell (e.g., the expression of cell surface
components and matrix material; Caiazza and O’Toole, 2004) and hydrophobicity and
charge of the substratum (Harkes et al., 1992; Mueller et al., 1992). Commitment, the
next phase, which involves “irreversible attachment”, is a crucial step in biofilm
formation since these initial colonizers form the foundation of the mature biofilm.
After this transition, cells cannot be removed from the surface by simple washing
procedures (Oliveira, 1992).
Following adhesion to a surface, bacterial cells aggregate, forming the basic structural
unit of a biofilm, referred to as a microcolony (Davey and O’Toole, 2000).
Microcolonies may form by one of three mechanisms - surface translocation, cell
recruitment and clonal growth. The first two mechanisms involve recruitment of new
cells to a microcolony. During surface translocation cells attached to the surface
utilize swarming or twitching motility to join existing microcolonies. In contrast cell
recruitment involves planktonic cells (Tolker-Nielsen et al., 2000) or cell flocs
(Stoodley et al., 2001) attaching directly to cell aggregates from the bulk fluid. In
clonal growth increase in microcolony size results from division of existing resident
bacteria. The relative contribution of each mechanism varies depending on the
organism involved, the surface being colonized and the environmental conditions
(Stoodley et al., 2002).
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 4
12 3 4
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During biofilm maturation the microcolonies reach their maximum dimensions. Cells
within a given microcolony are non-motile and are usually segregated into a number
of distinct cell clusters (Sauer et al., 2002). A microcolony is usually a simple conical
structure or mushroom-shaped. Microcolony structure is dependant upon the presence
of an extracellular cell-to-cell interconnecting matrix consisting mainly of
exopolymers (e.g. polysaccharides, proteins and DNA). In addition, outer membrane
proteins and cell appendages such as fimbriae, pili, and flagella may also form part of
the biofilm matrix (Pamp et al., 2007). The interconnecting matrix is interspersed
with highly permeable water-channels. These act as a “circulatory system,” delivering
nutrients and removing metabolic waste from the microcolony (Lawrence et al., 1991;
Costerton et al., 1994). Importantly biofilm growth form protects the biofilm-forming
organisms against the negative effects of antimicrobial agents and predation by
protozoans (Stewart, 2002; Matz and Kjelleberg, 2005). Additionally, biofilms
facilitate horizontal gene transfer and intracellular communication (Hausner and
Wuertz, 1999; Parsek and Greenberg, 2000) as well as promoting increased genetic
diversity of the bacterial populations (Boles et al., 2004). Such characteristics
improve the survival of bacterial communities in harsh environmental conditions.
For some bacteria, cell-cell communication is essential for the establishment of an
ordered biofilm community. Bacteria achieve this using secreted signalling molecules
called autoinducers in a process called “quorum sensing” (Nealson and Hastings,
1979). This enables the population to collectively regulate gene expression and,
therefore, behave as a group. Quorum sensing is known to control bioluminescence,
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 5
secretion of virulence factors, sporulation, and conjugation. Thus, quorum sensing is a
mechanism that allows bacteria to function much like a multi-cellular organism
(Hammer and Bassler, 2007).
As a biofilm matures dispersal of cell aggregates from the main body occurs. The
dispersal process may be either passive or active. Passive dispersal is a direct
consequence of the immediate environmental conditions and usually occurs by
erosion, sloughing, abrasion or predator grazing (Bryers, 1988). Cell aggregates are
released as a result of physical disruption of the biofilm. On the other hand active
dispersal mechanisms are used when environmental conditions become unfavourable.
In this case release of cells or cell aggregates is initiated and regulated by the biofilm.
For example, Pseudomonas spp., Escherichia coli, and Acinetobacter spp. biofilms
will release cells in response to nutrient starvation (Delaquis et al., 1989; Sawyer and
Hermanowicz, 2000; Jackson et al., 2002). Several studies have shown programmed
cell death is responsible for active dispersal. In Pseudoalteromonas tunicata the
antibacterial protein, AlpP, mediates cell death. This acts as a lysine oxidase resulting
in the production of hydrogen peroxidase and cell death within the microcolony (Mai-
Prochnow et al., 2004, 2006, 2008). Death of specific regions of the microcolony
results in the release of isolated cell aggregates. Phaeobacter gallaeciensis biofilms,
formerly Roseobacter gallaeciensis, also displays cell death within microcolonies
(Martens et al., 2006).
Cells dispersing from biofilms often exhibit phenotypic and genotypic variation, a
feature that is thought to enhance survival in the face of changing environmental
conditions and competitive regimes (Boles et al., 2004; Webb et al., 2004; Ho, 2008).
For example, dispersed cells of Ph. gallaeciensis express varying levels of
antimicrobial activity against the competitive colonizer, P. tunicata. This is expected
to lead to differential colonisation ability (Ho, 2008). In Pseudomonas aeruginosa
biofilms, small colony variants exhibit enhanced attachment and accelerated biofilm
development relative to the wild type strain (Webb et al., 2004).
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 6
1.1.3 Current biofouling control strategies and its impact on the marine ecosystem
To minimize the impact of biofouling on artificial structures in the marine
environment (e.g. ship’s hulls) many are protected with antifouling coatings. These
are paint-based and contain a biocide or toxin, often tributyl tin (TBT) or copper
based compounds (Thomas, 2001; Yebra et al., 2004). The biocide is slowly released
into the environment poisoning organisms that adhere to the surface.
However, since the biocides are non-specific they may also have harmful effects on
non-fouling organisms (Evans, 1999; Yebra et al., 2004). In the case of TBT, organo-
tin moieties are released as the coating degrades. These have a range of sublethal
effects on non-target species. For example, low concentrations of TBT may cause
defective shell growth in the oyster Crassostrea gigas and development of male
characteristics in female dog whelk Nucella lapillus (Evans, 1995). Perhaps most
alarming for the present study, studies indicate that the highest levels of TBT-
contamination have been recorded in Fiji, the most contaminated site recording a TBT
concentration of 360μgg-1 (Maata and Koshy, 2001).
Due to the non-specificity of TBT and other tin containing biocides in antifouling
paints, the International Maritime Organization and Marine Environmental Protection
Committee (MEPC) have banned their usage (Champ, 1999). This has prompted a
search for alternate antifoulants that are non-toxic and “environment-friendly.” An
understanding of the natural defence mechanisms of marine organisms against
biofouling is the first step towards “safer” antifoulants. It is hoped that these natural
defence strategies and the associated bioactive compounds may be manipulated to
develop novel antifouling technologies that are less harmful to the marine
environment.
1.1.4 Natural defence mechanisms against biofouling
Marine algae are also prone to biofouling. Seaweeds employ a number of physical
defence systems to prevent fouling. These include shedding of outer cell layers (Keats
et al., 1997), mucilaginous coverings on blades (Filion-Myklebust and Norton, 1981;
Moss, 1982) and continuous erosion of the distal ends of blades (Mann, 1973; Ott,
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 7
1980). Water turbulence and abrasion may also limit fouling (Sieburth and Tootle,
1981).
In addition, marine algae may produce inhibitory chemicals to prevent fouling and
grazing (Dworjanyn, et al., 1999). A well studied example is the red alga Delisea
pulchra, which produces an array of structurally related secondary metabolites known
as halogenated furanones (Kazlausks et al., 1977; de Nys et al., 1993). These
compounds interfere with bacterial colonization and prevent settling of invertebrate
larvae and the spores of common fouling algae (Kjelleberg et al., 1997; Maximilien et
al., 1998). Scanning electron microscopy of the alga reveals a significantly higher
abundance of epibacteria near the holdfast than closer to the blade apices (Steinberg et
al., 1997). This corresponds to a gradient in the concentration of halogenated
furanones - which are highest close to apices. Studies indicate that furanones may
control bacterial colonization by specifically interfering with acylated homoserine
lactone (AHL)-mediated gene expression at the level of the LuxR protein (Manefield
et al., 1999).
Although toxin mediated mechanisms are effective, they are energy expensive.
Generally, defence costs are the sum of (1) the energy and nutrients consumed for
defence production (and, therefore, lost to growth), (2) the energy necessary for
sequestering the toxins away from active cell processes, (3) the interference of the
defence with photosynthesis and (4) the loss of productivity from the tissue given it
would have photosynthesized if it were not co-opted for defence (Coley, 1986).
Hence, large amounts of energy are invested in toxin-mediated defence systems, and
this is costly for smaller and simpler algal forms.
Organisms that lack chemical or physical defences are thought to rely on secondary
metabolites produced by bacterial symbionts to provide defence against surface-
colonizing organisms (Armstrong et al., 2001; Berland et al., 1972; Thomas and
Allsopp, 1983). For example, symbiotic interactions have been found in the marine
crustaceans Palaemon macrodactylus and Homarus americanus where symbiotic
bacteria defend embryos from fungal infection (Gil-Turness and Fenical, 1992). More
generally, Holmstrom et al., (1996) investigated the frequency with which bacterial
strains isolated from living and inanimate surfaces displayed inhibitory activity
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 8
against fouling organisms. Results showed that 10% of isolates from rock surfaces
inhibited the settlement of invertebrate larvae compared with 30% of isolates from
marine animals and 74% from algal surfaces. These data suggest that many of the
bacteria that form epiphytic communities on living surfaces are able to regulate
fouling by other organisms (Egan et al., 2000).
Additionally, results from behavioral assays demonstrate that secondary metabolites
may be produced to ensure colonization by preferred epibionts (Wahl et al., 1994;
Bryan 1996; Engel et al., 2002). It is interesting to note that secondary metabolites
may control the density of surface associated microbes, allowing growth of a
community of preferred microbes rather than maintaining an axenic surface (Engel et
al., 2002). For example, in D. pulchra halogenated furanones affect bacterial
colonization differently. Attachment is inhibited in strains associated with surface-
fouling while growth and swarming is inhibited in the preferred strains (Maximilien et
al., 1998). The results explain why fouling strains are absent from the alga’s surface
and preferred bacterial strains have limited surface distribution.
The ecology of marine algal surfaces is known to be highly complex. As space and
nutrients are limited, colonization by bacteria often requires them to compete with one
another (Egan et al., 2008). Bacterial strains known to be associated with algal
surfaces include members of the Flavobacterium group of Bacterioidetes, members of
the Roseobacter clade (Rao et al., 2005) as well as various Pseudoalteromonas and
Alteromonas spp. (Holmstrom and Kjelleberg. 1999). Using a culture-independent
method, Longford et al. (2007) compared bacterial diversity on the red maccroalga D.
pulchra with that of U. australis. Approximately 79 species from 7 phyla were
isolated from D. pulchra while an estimated 36 species from only 4 phyla were
isolated from Ulva. Alpha-, Delta- and Gammaproteobacteria were all well
represented with Planctomycetes and Bacteroidetes common on both algae. However,
there were very few species common to both algae (Longford et al., 2007).
One of the major arguments for preserving biodiversity is the potential for discovery
of new bioactive compounds. For this reason, the genus Pseudoalteromonas has
received a lot of attention in the last two decades. The focus reflects the bacterium’s
frequent association with eukaryotic hosts in the marine environment. Studies of such
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 9
associations are useful for understanding the mechanisms underlying microbe-host
interactions. Also, many pigmented species of Pseudoalteromonas produce
biologically active metabolites (Egan et al., 2002b). Species of Pseudoalteromonas
display antibacterial, bacteriolytic, agarolytic and algicidal properties, as well as
various other pharmaceutically-relevant activities. Several Pseudoalteromonas strains
prevent the settlement and colonisation of marine surfaces by common fouling
organisms (Holmstrom and Kjelleberg, 1999; Bowman, 2007).
Within the genus, Pseudoalteromonas tunicata is thought to exhibit the broadest
range of inhibitory activities (Holmstrom et al., 2002). This species produces a
diverse range of biologically active compounds, many of which target marine fouling
organisms (Holmstrom et al., 1998). To date a range of antifouling compounds have
been isolated from P. tunicata. The antifungal compound is a yellow, tambjamine-like
alkaloid (YP1), the biosynthetic pathway of which is encoded by a cluster of 19 genes
(tamA to tamS; Franks et al., 2005; Burke et al., 2007). Moreover, the autolytic
antibacterial protein (AlpP) produces hydrogen peroxide which causes cell death,
mediates differentiation, dispersal and phenotypic variation during the dispersal event
(James et al., 1996; Mai-Prochnow et al., 2004, 2008). Other bioactive compounds
include a polar, heat-stable anti-larval molecule (Holmstrom et al., 1992), a heat-
sensitive anti-algal peptide (Egan et al., 2001) and an uncharacterized anti-diatom
compound. With such a wide range of antifouling characteristics present in P.
tunicata, the antifouling potential of the remainder of the genus is worth investigating.
More knowledge of the biologically active chemicals produced by
Pseudoalteromonas would also be potentially pharmacologically beneficial (Bowman,
2007).
The Roseobacter clade is another group of marine bacteria that due to its worldwide
distribution, abundance and physiological diversity is well studied (Brinkhoff et al.,
2008). The group has been isolated from both coastal and open waters, a variety of
micro- and macro-algae, microbial mats, sediments, polar sea ice, and marine
invertebrates (Buchan et al., 2005; Wagner-Dobler and Biebl, 2006). Members of the
group often form symbioses with higher organisms (Bruhn et al., 2007). For example,
the symbiotic association between Silicibacter sp. strain TM1040 (a member of the
Roseobacter clade) and the dinoflagellate Pfiesteria piscicida involves bacterial
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 10
chemotaxis to dinoflagellate-produced dimethylsulfoniopropionate (DMSP), DMSP
demethylation, and ultimately a biofilm on the surface of the dinoflagellate host
(Alavi et al., 2001; Miller and Belas, 2004; Miller et al., 2004). Biofilm formation
coincides with the production of an antibiotic, a sulfur-containing compound,
tropodithietic acid (TDA). Since the genes critical for TDA biosynthesis are located
on plasmids in both Silicibacter sp. strain TM1040 and Phaeobacter sp. strain 27-4, it
is suggested that both members of the Roseobacter clade may use a common pathway
for TDA biosynthesis that involves plasmid-encoded proteins (Geng et al., 2008).
This suggests that investigating other members in the Roseobacter clade for bioactive
properties is important.
Phaeobacter gallaeciensis (a member of the Roseobacter clade) is a commonly
studied temperate, biofilm-forming strain. Together with Pseudoalteromonas
tunicata, Ph. gallaeciensis benefits its algal host by producing compounds that inhibit
common fouling organisms. Studies have shown Ph. gallaeciensis to be more
competitive than P. tunicata during biofilm formation and having the capacity to
invade and disperse pre-established biofilms (Rao et al., 2006). Hence, given strong
competitive characteristics, participation in symbiotic interactions with eukaryotic
hosts and wide distribution, members of the Roseobacter clade are also strong
candidates for future antifouling solutions.
While it is acknowledged that the technology available to assess and exploit microbial
diversity is limited, there is a need for studies that will enhance current understanding
of microbial associations (Egan et al., 2008). It is recognized that many of the marine
invertebrates (e.g. sponges, bryozoans and tunicates) that are sources of secondary
metabolites also contain endo- and epibiotic microorganisms. Indeed, some
invertebrate-derived natural products are structurally related to the bacterial
metabolites (Sudek et al., 2007). With the complexity of associations in marine
organisms, it is difficult to determine the biosynthetic source of many marine natural
products (Konig et al., 2006). However, it is now recognised that many of these
metabolites may well be of microbial origin (Sudek et al., 2007). The marine
bryozoan Bugula neritina synthesizes bryostatins, complex polyketides that render the
B. neritina larvae unpalatable to predators (Sharp et al., 2007). A recent study has
shown that bryostatin, isolated from B. neritina, is actually produced by the
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 11
uncultured symbiotic bacterium “Candidatus Endobugula sertula" (Sudek et al.,
2007). The finding highlights the important role of biotechnological advancement in
the discovery and exploitation of microbial defence mechanisms. The need was
recently re-emphasized when for the first time a strain of the Roseobacter clade-
affiliated (RCA) cluster was successfully isolated and propagated (Mayali et al.,
2008). This was accomplished through the application of novel techniques with algal
cultures. Previous efforts to culture the RCA cluster as well as many other bacteria
abundant in the marine environment, using traditional culture methods have not been
successful. This recent finding stresses the need for developing novel molecular
approaches to study uncultivated microbial diversity which could potentially lead to
the discovery of new compounds (Egan et al., 2008) and improved biofouling-control
techniques.
1.2 Diatoms as marine surface colonisers
Like bacteria, diatoms are also an important constituent of microfouling communities
on marine surfaces. However, most studies have focused on the bacterial component.
In the current search for improved-control strategies, it is essential to also develop an
understanding of the role that diatoms play. This will be critical for finding more
effective means of tackling the issue of biofouling.
1.2.1 Diatom biology
Diatoms are among the earliest eukaryotic colonizers of submerged surfaces and are
among the most conspicuous components of natural biofilms (Evans 1988). Diatoms
belong to the Bacillariophyceae with over 250 genera and perhaps as many as 100,000
species (Norton et al., 1996; Van Den Hoek et al., 1997). Characteristically, the cell
walls are highly patterned with pores and ridges. They are unique among the algae
due to the presence of silica-based cell walls. Most diatoms contain silicon
transporters (SITs) for transferring Si(OH)4 across lipid bilayer membranes
(Hildebrand et al., 1997). Diatoms take up silicon predominantly as silicic acid that is
then polymerized and deposited into the cell wall as silica (Del Amo and Brzezinski,
1999). Silicic acid is co-transported with sodium in marine diatoms with zinc also
suggested to play a role in silicic acid uptake (Sullivan, 1977; Rueter and Morel,
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 12
1981). The diatom of interest in this research is Cylindrotheca fusiformis. This
autotrophic, marine, pennate diatom is being used as a model organism for studying
transport, deposition and patterning of silica in diatom cell walls. Biosilica from all
diatom species investigated so far has shown to be a composite material containing
proteins (mainly the silaffins) and long-chain polyamines as organic components.
These organic constituents have been recognised as important players in silica
biomineralisation. Several recent reviews have described the structure and properties
of these organic molecules (mainly from C. fusiformis) as well as possible function in
silica formation and patterning (Pohnert, 2002; Foo et al., 2004; Sumper et al., 2004;
Sumper and Brunner, 2006).
The wall is constructed of two sections or thecae, with the smaller hypotheca fitting
within a larger epitheca much like a Petri dish (Figure 1.3). In diatoms one of the most
important cell wall proteins is pleuralin, which is involved in the cell cycle-dependent
frustule development. To maintain the integrity of the frustule, coupling between
biogenesis of new frustule components and cell cycle is required. The molecular
mechanism by which this coupling occurs is unknown. Interestingly, although the
thecae are morphologically similar, immunolocalisation with anti-pleuralin antibodies
demonstrates that their protein composition is clearly different (Kroger and
Wetherbee, 2000). It is hypothesized that pleuralins are involved in hypotheca-
epitheca differentiation, a crucial process that ensures proper frustule development.
(Redrawn from Hasle and Syvertsen, 1997)
Centric Diatoms Pennate Diatoms
Diagrammatic section showing frustule terminology
epivalve
valve view girdle viewvalve view girdle view
epetheca
hypotheca
hypovalve
����������� ����� ������������������� �����������������������������
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 13
Generally, two types of diatoms are recognised, pennate or bilaterally symmetrical
diatoms and centric or radially symmetrical diatoms. The former are mostly
planktonic and the latter predominately benthic, associated with sediments or attached
to rocks or macroalgae (Falciatore and Bowler, 2002; Leblanc et al., 1999). Diatoms
can be unicellular or colonial and either autotrophic or heterotrophic (Gilabert, 2007).
The brown colour of diatoms is due to the presence of the carotenoid pigment
fucoxanthin, which is located together with chlorophyll a and c in their plastids
(Round and Crawford, 1990). Reproduction in diatoms is mainly asexual, the
daughter cells each receiving one half of the parental cell wall and constructing a new
frustule half within it (Raven et al., 1999). Benthic diatoms are able to glide along
surfaces; mucilage is secreted into furrow (known as a raphe) which allows movement
(Falciatore and Bowler, 2002). In contrast, most planktonic diatoms are non-motile
and rely on mixing of the water column to remain suspended (Stoermer et al., 2004).
1.2.2 Diatom adhesion, motility and extracellular polymeric substances
Diatoms are abundant in benthic habitats where they adhere to surfaces using copious
quantities of mucilage. Depending on the nature of the surface, initial contact may or
may not result in bonding by the diatom (Wetherbee et al., 1998). Adhesion in
diatoms is Ca2+ dependent and the process requires metabolic energy, protein and
glycoprotein synthesis (Cooksey and Wigglesworth-Cooksey, 1995). Thus diatom
bonding requires an active commitment involving the activation of specific adhesion
mechanisms. In most benthic diatoms, cell-substratum adhesion occurs at the raphe,
resulting in cell reorientation and a unique form of cell motility called “gliding”
(Edgar and Pickett-Heaps, 1984). The mucilage secreted into the raphe links the cell
cytoplasm to the substratum. This provides for 'gliding' motility via an actin-myosin
system located adjacent to each raphe (Edgar and Pickett-Heaps, 1984; Poulsen et al.,
1999). Cell-substratum adhesion at the raphe is a requirement for diatom gliding
(Edgar and Pickett-Heaps, 1984; Wetherbee et al., 1998). As diatoms glide, the
secreted mucilaginous strands are detached and left behind as diatom “trails” that
eventually accumulate as a component of biofilms (Edgar and Pickett-Heaps, 1984;
Higgins et al., 2000; Wetherbee et al., 1998). In addition, the trails remain adhesive
and may aid in the accumulation of other biofouling agents (Lind et al., 1997).
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 14
The mucilage or extracellular polymeric substance (EPS) is produced by benthic
diatoms both as part of the motility system and as a response to environmental
conditions. The EPS is composed of polysaccharides, proteins, and glycoproteins
(Chiovitti et al., 2003). Typically carbohydrates are the dominant component of EPS,
but the constituent sugars are often complex and highly diverse (Hoagland et al.,
1993). Characterization of EPS structure, serology, and lectin interactions, provides
for a broad classification of EPS materials. Several subtypes are recognized including
frustule EPS, outer capsular EPS, motility EPS, and matrix EPS (Wigglesworth-
Cooksey and Cooksey, 2005). Combined, diatoms and their insoluble EPS are
common features of biofouling communities.
1.3 Aims of this study
The green alga Ulva spp. does not produce secondary metabolites with recognised
roles in fouling prevention (Awad, 2000; Abd El-Baky et al., 2008). Ulva spp. is
found in temperate and tropical waters, including the shores of Fiji. While
antibacterial activities have been identified for epiphytic bacteria isolated from
temperate Ulva spp., the occurrence of anti-diatom properties has been less
intensively investigated. The latter is likely due to the inherent, technical challenges
of performing anti-diatom bioassays.
The major hypothesis addressed in this study is that surface-associated bacteria from
tropical Ulva spp. have characteristics that have a role in limiting surface fouling of
the algae. First the study aimed to isolate epiphytic bacteria from Fijian collection of
Ulva spp. growing in tropical Fiji waters and characterise their inhibition of bacteria
and diatoms. The second part concentrated on the prevalence of anti-diatom activity
across two ecologically significant bacterial groups, namely Pseudoalteromonas and
the Roseobacter clade. A further focus was the anti-diatom strategy of the model
epibiont, P. tuncata, with gene identity information used to propose a preliminary
model describing the mechanism.
Chapter 1: Introduction
Inhibition of primary colonizers by marine surface-associated bacteria 15
To address the hypothesis the specific aims of this study were to:
1. Isolate and assess inhibitory activity of the epibionts against bacteria and
diatoms.
2. Identify the taxonomy of the epibionts with inhibitory properties and establish
a correlation with previous studies.
3. Screen Pseudoalteromonas and Roseobacter strains for anti-diatom activity.
4. Identify potential genes involved in the expression of the anti-diatom
compound produced by P. tunicata and suggest a hypothetical model to
describe the mechanism.
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 16
Chapter 2: Inhibitory activity of epiphytic bacteria isolated
from Ulva
2.1 Introduction
Marine macroalgae are prone to colonization by fouling organisms. To limit fouling,
some macroalgae produce secondary metabolites that mediate intra- and interspecific
interactions (Harborne, 2001; Rosenthal and Berenbaum, 1992). Although such
chemical defences are effective, they are expensive in terms of the energy required for
metabolite production (Thomas, 2001). Instead simpler algal forms are suggested to
have alternative mechanisms to prevent surface fouling.
Some bacteria produce inhibitory compounds that prevent surface fouling. Algae that
lack physical or chemical defence mechanisms are thought to form symbioses with
these bacteria (Holmström and Kjelleberg, 1999; Rao et al., 2005; Longford et al.,
2007). Various studies show that epiphytic bacteria on marine surfaces display
inhibitory activity against fouling organisms (Armstrong et al., 2001; Berland et al.,
1972; Thomas and Allsopp, 1983; Holmstrom et al., 1996). For example, Lemos et
al., (1985) isolated epibionts from five species of green and brown algae and found
that 38 of 224 isolates displayed antibacterial activity.
Bacteria of the Flavobacterium group, various Pseudoalteromonas and Alteromonas
spp. (Holmstrom and Kjelleberg. 1999) and members of the Roseobacter clade (Rao
et al., 2005) are commonly found on marine surfaces. Amongst these bacteria,
Pseudoalteromonas is unique. Fairly recently, the genus was established to contain
various species that produced biologically active molecules (Holmstrom and
Kjelleberg, 1999). In particular P. tunicata has the ability to influence the behaviour
of higher organisms (Holmstrom et al., 1998). Another ecologically important group
is the Roseobacter clade. The group includes the species Phaeobacter gallaeciensis,
frequently isolated from the surface of U. australis (Shiba, 1992), marine snow
particles (Gram et al., 2002) and dinoflgellates (Alavi et al., 2001; Lafay et al., 1995;
Miller and Belas, 2004). The bacterium demonstrates antibacterial activity (Brinkhoff
et al., 2004; Rao et al., 2005; Ruiz-Ponte et al., 1998). Advancement of current
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 17
biofouling-control strategies depends on the study of such inhibitory epiphytic
bacteria which may lead to the discovery of new bioactive compounds.
Much is already known about the antibacterial, anti-algal and anti-larval properties of
surface colonizing bacteria. However, anti-diatom capacity remains largely
unexplored. Diatoms are amongst the early colonizers of marine substrates and are
important components of the biofouling community. The lack of study largely reflects
lack of suitable culture techniques of diatoms in bioassay screens.
The green algae, Ulva spp. does not produce secondary metabolites with recognised
roles in fouling prevention (Awad, 2000; Abd El-Baky et al., 2008) but does play host
to antifoulant producing bacteria (Holmstrom et al., 1996; Lemos et al., 1985). Hence
the alga is a suitable model system for exploring the role of inhibitory bacteria. Ulva
is a cosmopolitan chlorophyte and found in temperate and tropical waters, including
the shores of Fiji. Compared to temperate climates, tropical conditions may support a
greater microbial diversity, but this remains unexplored. The study aimed to
investigate whether Ulva growing in Fiji waters had surface microflora similar to that
of temperate waters, which it relied upon for the prevention of surface fouling. The
approach was to test isolated bacteria for inhibitory activity against both bacteria and
diatoms. The epibionts with inhibitory properties were taxonomically classified and
correlated with previous studies.
2.2 Materials and methods
2.2.1 Isolation of epiphytic bacteria from Ulva
Samples of the green algae Ulva, were randomly collected from the intertidal zone of
Laucala Bay, Suva, Fiji (18°06'S, 175°30'E). Collections were made at low tide and
samples stored in sterile polyethylene bags for transport to the laboratory. The algal
samples were washed with sterile seawater to remove loosely attached bacteria. To
isolate bacteria that were tightly bound to the algal surface, samples were placed in
vials containing 10 ml of sterile seawater and vortexed for 5 min. Aliquots of the cell
suspensions were used to inoculate marine agar (Difco marine broth solidified with
1.5% agar) which were then incubated at 23°C for 48 hr. Morphologically distinct
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 18
bacterial colonies were selected and stored at -80°C in 30% glycerol (v/v). Isolates
were routinely grown and maintained on marine agar at 23°C.
2.2.2 Bioassay against growth of bacteria
Bacteria isolated from the surface of Ulva were tested for antibacterial activity
alongside three common laboratory strains; E. coli, Pseudomonas aeruginosa PAO1
and Bacillus strain CC6 (culture collection, Centre for Marine Bio-Innovation,
University of New South Wales, Australia). The antimicrobial assay was modified
from Rao et al., (2005). Broth cultures of algal isolates were grown for two days at
room temperature (23°C) and the supernatant isolated by centrifugation at 13 000 × g
for 5 min. Supernatant samples were assayed for inhibitory activity using the drop
assay. Briefly, 100 μl of 48 hr old target marine isolate and 24 hr old target laboratory
isolate were spread on marine agar plates, and the plates were dried at 30°C for 30-60
min. Drops containing 10 μl of the test isolate supernatant, as well as a control
(uninoculated marine broth) were placed on the agar surface and incubated at room
temperature (23°C) for two days to allow formation of inhibition zones. Assays were
conducted in triplicate.
2.2.3 Bioassay against growth of diatoms
The effect of the bacterial isolates on diatom growth was assessed using the pennate
diatom, Cylindrotheca fusiformis, (CSIRO microaglae culture collection, Hobart,
Australia). C. fusiformis was chosen as the target diatom as it grows rapidly on agar
plates (Chan et al., 1980). Diatoms were subcultured routinely by aseptically
transferring 5 ml of the inoculum to 100 ml of the diatom culture solution-f/2
(Guillard and Ryther, 1962; Appendix I) and incubating at 20°C. A photoperiod of 16
hr light: 8 hr dark was provided (as per supplier’s instructions).
To determine inhibitory activity, the diatom plating assay (Chan et al., 1980) was
used with some modifications. Briefly, 300 μl of exponential phase diatom culture
(with optical density of higher than 0.06, at 600nm) was spread evenly over the
surface of marine agar (Difco marine broth solidified with 1.5% agar) using a sterile
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 19
glass spreader and allowed to dry. The bacterial test culture was transferred to the
centre of inoculated plates by spotting with an inoculating loop. Plates were incubated
inverted at 20°C with a photoperiod of 16 hr light: 8 hr dark. Light was provided both
from above and below the plates. Growth was monitored over 4 days. Anti-diatom
activity was indicated by the presence of growth inhibition zones. Plates inoculated
with diatom cultures only, served as a control for diatom growth. Assays were
conducted in triplicate.
2.2.4 Identification of isolates with inhibitory properties
2.2.4.1 DNA extraction
DNA was extracted from bacterial isolates with inhibitory activity against bacteria
and diatoms. Extractions were conducted using the XS-buffer method (Tillett and
Neilan, 2000; Appendix I). A 2 ml aliquot of a 2 day old culture was pelleted by
centrifugation, the supernatant discarded, and cells subsequently resuspended in 1 ml
of XS-buffer. The suspension was incubated at 70°C for 60 min. After incubation,
tubes were vortexed for 10 sec and placed on ice for 30 min. Tubes were then
centrifuged at 21 000 × g for 10 min. The supernatant was transferred to a clean 2 ml
microcentrifuge tube, 1 volume of isopropanol was added and the solutions mixed.
The tubes were incubated at room temperature for 5 min and then centrifuged at
21000 × g for 10 min. The supernatant was decanted and the pellet washed with 70%
(v/v) ethanol. The pellet was then air dried before being resuspended in 50-100 μl of
sterile deionised water.
2.2.4.2 Agarose gel electrophoresis
The extracted DNA was examined by electrophoresis on 1% (w/v) agarose gel using
�-DNA digested with EcoRI/HindIII as a size marker and for concentration
estimation. Gels were run in 1 × TBE buffer (Appendix I) at 80 volts for 20-30 min,
stained with ethidium bromide, destained in TBE buffer, and then photographed using
the Gel-Doc Imaging system (BioRad).
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 20
2.2.4.3 PCR amplification of 16S rRNA gene
The 16S rRNA gene was amplified using the polymerase chain reaction (PCR).
Reaction volumes of 20 μl contained 1 × PCR Reaction Buffer (Invitrogen), 250 μM
of each deoxynucleotide triphosphate (dNTP), 25 pmol of each of F27 and R1492
primers (Appendix II), 2.5 mM MgCl2 (Invitrogen), 0.05 unit Platinum Taq DNA
Polymerase (Invitrogen) and 10 ng of extracted DNA template. Reaction mixture was
thermocycled as follows: 30 cycles of denaturation at 94°C for 30 sec, annealing at
50°C for 30 sec and extension at 72°C for 2 min. A final extension step was
performed at 72°C for 5 min and samples were held at 4°C.
PCR product concentration was estimated by agarose gel electrophoresis as described
in section 2.2.4.2. For successful amplifications, the PCR product was purified using
QIAquick PCR Purification Kit as per manufacturer’s instructions. Purified products
were examined using gel electrophoresis as described above (section 2.2.4.2.).
2.2.4.4 DNA sequencing and sequence analysis
The purified PCR product were sequenced unidirectionally using 25 pmol of either of
F27 or R1492 primers (Appendix II), 20 ng of DNA template, 5 × CSA sequencing
buffer (Applied Biosystems), 1 unit of BigDyeTM terminator cycle sequencing
reaction mix v.3.1 (Applied Biosystems) and sterile deionised water in a final volume
of 20 μl. Cycle sequencing was conducted using the following thermoprofile: 94°C
for 10 sec, 50°C for 5 sec and extension at 60°C for 4 min in 99 cycles. Extension
products were purified by ethanol precipitation. Specifically, 5 μl of 125 mM EDTA
and 60 μl of 100% ethanol were added to each reaction tube and vortexed briefly. The
extension products were left to precipitate for 30 min at room temperature. Tubes
were then centrifuged at 21 000 × g for 20 min and the supernatant aspirated. The
pellet was washed twice with 70% ethanol (v/v), the tubes briefly vortexed and
centrifuged at 4°C, at 21 000 × g for 10 min. Samples were dried in a speedvac for 15
min. Sequencing was performed on an ABI 3730 DNA sequencing system at the
Automated Sequencing Facility, UNSW. Sequences obtained were compared to
sequences available in the NCBI BLAST 2.0 database (Altschul et al., 1990).
Phylogenetic analysis was performed using the sequence data software, ARB (Ludwig
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 21
et al., 2004) and the Greengenes database (DeSantis et al., 2006). Specifically,
sequences were aligned to the Greengenes database in ARB using the integrated
aligner. The sequence alignments were manually checked and redefined, if necessary.
Placement of the sequences in the phylogenetic tree was determined by the maximum
parsimony algorithm implemented in ARB. Taxonomic assignment was based on
closely-related strains in the tree and the Hugenholtz taxonomy included in the
Greengenes database. In addition, taxonomic classification was also undertaken by the
Ribosomal Database Project II classifier based on a naïve Bayesian rRNA classifier
(Wang et al., 2007).
2.3 Results
2.3.1 Epiphytic bacteria isolated from Ulva
Temporal replicates of culturing efforts from Fijian Ulva spp. yielded different
bacterial morphotypes, of which 14 could be routinely sub-cultured. Using colony
morphology and Gram staining, redundant isolates were eliminated. A total of 10
distinct bacterial isolates were chosen and used for further experiments.
2.3.2 Production of extracellular antibacterial compounds
Bacteria isolated from Ulva along with laboratory strains were used as target strains in
assessing antibacterial activity of the Ulva epibionts. Table 2.1 summarizes the effect
of epiphytic bacteria on the growth of 13 bacterial strains. Of the 10 isolates, 60%
expressed some inhibitory action. The broadest ranges of antibacterial activity were
displayed by U15 and U11, which were effective against 50% and 33% of the target
strains, respectively. Isolates U8, U12, U13 and U14 failed to inhibit the growth of any
of the bacterial strains tested.
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 22
2.3.3 Growth inhibition of diatoms
The effect of the 10 isolated epiphytic bacteria on the growth of C. fusiformis is
summarized in Table 2.2. Eight of the ten isolates showed inhibitory activity against
C. fusiformis. Isolates U7, U11 and U15 were the most effective whereas isolates U1 and
U12 had no effect on C. fusiformis.
Table 2.1: Antibacterial activity expressed by bacteria isolated from Ulva
Target
Strain
Bacterial Isolate
U1
(mm)a
U3
(mm)
U4
(mm)
U7
(mm)
U8
(mm)
U11
(mm)
U12
(mm)
U13
(mm)
U14
(mm)
U15
(mm)
U1 * 1 0 0-1e 0 0-1e 0 0 0 0-1e
U3 0 * 0 0 0 0 0 0 0 0-1e
U4 0 0 * 0 0 0-1e 0 0 0 0
U7 0 0 0 * 0 0-1e 0 0 0 0-1e
U8 1 1-2 0-1e 0 * 0-1e 0 0 0 0-1e
U11 0 0 0 0 0 * 0 0 0 0
U12 0 0 0 0 0 0 * 0 0 0
U13 0 0 0 0 0 0 0 * 0 0
U14 0 0 0 0 0 0 0 0 * 0
U15 0 0 0 0 0 0 0 0 0 *
E. colib 0 0 0 0 0 0 0 0 0 0
PAO1c 0 0 0 0 0 0 0 0 0 1
CC6d 0 0 0 0 0 0 0 0 0 2
*Autoinhibitory activity was not tested. a The radius of growth inhibition measured in millimetres. b Escherichia coli c
Pseudomonas aeruginosa PAO1 d
Bacillus strain CC6
e Growth inhibition radii of a value greater than zero and less than one millimetre.
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 23
Table 2.2: Inhibition of C. fusiformis as expressed by bacteria isolated from Ulva
Bacterial Isolate Inhibition Zone Radii (mm)*
U1 0
U3 0-1a
U4 0-1a
U7 0-2b
U8 0-1a
U11 0-2b
U12 0
U13 0-1a
U14 0-1a
U15 0-2b
*The radius of growth inhibition measured in millimetres. a Growth inhibition radii of a value greater than zero and less than one millimetre. b Growth inhibition radii of a value greater than zero and less than two millimetres.
2.3.4 Characterization of active bacterial strains
On the basis of screening results, 8 active strains were chosen for species
identification. Table 2.3 summarises the identity of the isolates based on comparison
to NCBI, Ribosomal Project and ARB Project databases. Isolates were found to have
high identity (99-100% base identity) with those of previously sequenced marine
bacteria. Phylogenetic relations of the isolates to their closest groups are given in
Figures 8.1-8.6 (Appendix III).
Cha
pter
2: I
nhib
itory
act
ivit
y of
epi
phyt
ic b
acte
ria
isol
ated
fro
m U
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Inhi
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on o
f pr
imar
y co
loni
zers
by
mar
ine
surf
ace-
asso
ciat
ed b
acte
ria
24
Tab
le 2
.3: 1
6S r
RN
A g
ene
iden
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.218
Cha
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2: I
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Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 27
2.4 Discussion
2.4.1 Antibacterial activity of bacterial isolates
Antibacterial activity is known to be present in many surface-associated bacteria
(Holmström and Kjelleberg, 1999; Rao et al., 2005; Longford et al., 2007). Many
isolates in this study also displayed antibacterial activity (Table 2.1). Additionally,
U15 which inhibited the largest number of isolates was pigmented. This correlates
with a previous study where pigmentation was linked to the production of antifouling
compounds. The study by Egan et al., (2002b) observed that colour mutants of P.
tunicata differed in antifouling characteristics. Moreover, loss of antifouling activities
and pigmentation was the result of disruption to genes with sequence similarities to
transcriptional regulators, ToxR from Vibrio cholerae and CadC from Escherichia
coli (Egan et al., 2002a).
During colonization, epiphytic bacteria compete for space and nutrients. Having
antimicrobial properties confers selective advantages during colonization. It also
provides protection to the host by reducing colonization of fouling organisms.
Numerous studies show that bacteria produce active compounds against other
microorganisms as well as against higher organisms (Egan et al., 2000; Kjelleberg et
al., 1997). This characteristic may contribute to the overall microbial diversity on an
algal surface since colonization and settlement of other organisms becomes highly
regulated. Generally, a multitude of factors such as chemical-mediated interactions,
communication, space and nutrient limitation and competition may shape the
composition and properties of a surface community (Egan et al., 2008).
2.4.2 Anti-diatom activity of bacterial isolates
Anti-diatom activity was observed to occur widely amongst the bacterial isolates
(Table 2.2). The presence of growth inhibition zones on assay plates may indicate the
production of inhibitory substances by these isolates. A few studies have investigated
anti-diatom activity in marine bacteria. Silva-Aciares and Riquelme (2007) recently
studied the effect of bacterial biofilms of Alteromonas sp. strain Ni1-LEM on the
settlement of 8 marine benthic diatoms. Comparison was made against Halomonas
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 28
marina (ATCC 25374) and Pseudoalteromonas tunicata, reference strains with
proven antifouling properties. The highest antifouling activity was found for the
Alteromonas strain. Similarly, a study of diatom settlement responses to crude
extracts of several sponge species linked laboratory results with field evidence. In the
laboratory, 6 out of 7 sponge extracts inhibited growth and caused mortality of the
pennate diatom Nitzschia paleacea at tissue-level concentration. For field
experiments, sponge metabolites immobilized in a gel matrix were exposed to natural
microbial communities. After 7 days of exposure, 6 extracts suppressed the
recruitment of diatoms (Dobretsov et al., 2005). These results indicate that anti-
diatom activity is a common feature of marine surface-associated organisms.
However, lack of suitable assay techniques has limited diatom-related studies.
The ecological significance of anti-diatom activity may be that bacteria are able to
symbiotically exist with the host by preventing settlement and growth of diatoms in
exchange for space and nutrients. Additionally, bacteria with the ability to inhibit
diatom growth may be at an advantage during colonization with more effective
isolates being more competitive than other surface colonizers.
2.4.3 Identification of active bacterial strains
Most of the isolates characterised in this study share sequence similarity to surface-
associated marine bacteria previously isolated from temperate habitats. The majority
of the isolates in the present study fall within the Proteobacteria (Table 2.3), a finding
consistent with the global distribution of this group (Britschgi and Giovannoni, 1991;
Schmidt et al., 1991; Field et al., 1997). As noted by Longford et al., (2007)
comprehensive studies have led to the recognition of bacterial distribution in
planktonic communties. In contrast, the study of living surface-associated biofilms is
still in its infancy. Hence there is insufficient data to make similar large-scale
comparisons of epibionts.
Several studies have looked at the diversity of bacteria on Ulva (Longford et al.,
2007; Skovhus et al., 2007; Egan et al., 2000). Using a culture-independent method,
Longford et al., (2007) found bacteria from an estimated 36 species and 4 phyla
present on the surface of U. australis. These included Alpha-, Delta- and
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 29
Gammaproteobacteria along with Planctomycetes and Bacteroidetes. Moreover,
bacteria of the genus Pseudoaltermonas has also been isolated from the surface of
Ulva (Skovhus et al., 2007; Egan et al., 2000). In addition, a study showed that
bacterial cells on the surface of U. australis consisted of approximately 70%
Alphaproteobacteria and 13% Cytophaga-Flavobacteria (Tujula, 2006). In this study,
except for one isolate, all were identified as Gammaproteobacteria.
It is speculated that expertise in culture-independent studies may be useful for
demonstrating a greater microbial diversity on tropical Ulva spp. that has potential for
more antifouling activities. Since marine bacteria have low culturability and are slow
growing, cell recovery may be increased by increasing incubation period. In addition,
using alternative media (e.g. a polysaccharide containing marine medium with a
variety of substrates such as sea salts) could lead to the isolation of a wider range of
bacteria.
Two inhibitory isolates (U4 and U8) had highest sequence similarity with Shewanella
sp. (Table 2.3; Figures 8.2 and 8.4, Appendix III). Isolate U4 showed 100% similarity
to Shewanella oneidensis SCH0402, Genbank accession AY881235. This bacterium
was originally isolated from temperate South Korean waters. The strain was found to
be most active against a range of target bacteria and to have stronger repellent activity
than tributyltin oxide (Bhattarai et al., 2006). Two antifouling compounds have been
isolated from Shewanella oneidensis SCH0402, identified as 2-hydroxymyristic acid
and cis-9-oleic acid (Bhattarai et al., 2007). These may or may not be the same
compounds responsible for antifouling activity observed in this study. Isolate U8 also
showed high sequence similarity (99%) to Shewanella sp. However, based on
phylogenetic analysis on the ARB database, U8 appeared to be a different species to
U4 (Figures 8.2 and 8.4, Appendix III).
Also identified in this study were 3 isolates (U7, U11, and U15) belonging to the genus
Pseudoalteromonas (Table 2.3; Figures 8.3 and 8.6, Appendix III). Bacteria of the
genus Pseudoalteromonas are often present on the surface of Ulva spp. (Egan et al.,
2000; Skovhus et al., 2007). Pseudoalteromonas sp. influence biofilm formation in
various marine niches; are involved in predator-like interactions within the microbial
loop; influence settlement, germination and metamorphosis of various invertebrate
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 30
and algal species; and are adopted by marine flora and fauna as defence agents
(Bowman, 2007).
Pigmented species of Pseudoalteromonas produce an array of both low and high
molecular weight compounds with anti-fouling activities. The compounds formed
include toxic proteins, polyanionic exopolymers, substituted phenolic and pyrolle-
containing alkaloids, cyclic peptides and a range of bromine-substituted compounds
(Bowman, 2007). In the current study, isolate U15, that had 100% sequence similarity
with Pseudoalteromonas rubra, was also red-pigmented and had the strongest
antibacterial and antidiatom activities (Tables 2.1 and 2.2). The bright red pigment of
P. rubra, is a low molecular weight substance, identified as cycloprodigiosin HCl
(Gerber and Gauthier, 1979; Kawauchi et al., 1997). This compound is of
pharmaceutical importance as an immuno-proliferation suppressesor (Magae et al.,
1996), for displaying anti-malarial activity (Kim et al., 1999) and for inducing
apoptosis in several cancer cell lines (Campàs et al., 2003; Perez-Tomas et al., 2003).
Substituted phenylalkenoic acids, referred to as rubrenoic acids, purified from P.
rubra show bronchodilatatoric activity. P. rubra also forms a high molecular weight
substance, which is possibly a glycoprotein or polysaccharide known to expresses
antibacterial activity. Growth inhibition by the antibiotic is due to the induction of
oxidative stress in target cells through increased O2 uptake and an accumulation of
hydrogen peroxide (Gauthier, 1976a; b). Currently there are no reports of anti-diatom
activity in P. rubra and either of the known bioactive molecules or a new molecule
may be responsible for the antidiatom characteristic of the bacterium. Isolates U7 and
U11 had respectively 99% and 100% sequence similarity to Pseudoalteromonas sp.
Moreover, phylogenetic analysis showed that the two isolates are possibly closely
related (Figure 8.3; Appendix III).
Two of the bacterial isolates (U13 and U14) were identified as members of the genus
Vibrio (Table 2.3; Figure 8.5, Appendix III). Phylogenetic analysis showed that the
two isolates may be closely related (Figure 8.5; Appendix III). Isolate U13 had closest
sequence similarity (99%) to Vibrio sp. A356, Genbank accession DQ005876. This
bacterium was originally isolated from the surface of coralline algae. The isolate
induced larval settlement in the common Australian sea urchin Heliocidaris
erythrogramma (Hugget et al., 2006). In another study, a Vibrio sp. isolated from
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 31
Ulva reticulata, growing in Hong Kong waters inhibited settlement and
metamorphosis of the polychaete Hydroides elegans larvae (Dobretsov and Qian,
2002). Such findings suggest that Vibrio spp. live in close association with algal
surfaces and may either play an inhibitive or inductive role. The results of this study
correlate with findings of Dobretsov and Qian (2002), highlighting inhibitory
characteristics of Vibrio spp. Prior to the results presented here, antidiatom activity in
Vibrio spp. have not been reported.
Isolate U3 had activity against C. fusiformis and was identified as having closest
sequence similarity (99%) to Bacillus sp. (Table 2.3; Figure 8.1, Appendix III). The
general understanding of marine bacterial diversity gained from planktonic and
epiphytic communities suggest that the majority of isolates are Gram-negative
(Farmer and Hickman-Brenner, 1992). Also, recent culture-independent studies of
bacterial diversity on the surface of Ulva spp. have not reported the presence of
Bacillus sp. (Tujula, 2006; Longford et al., 2007). However, there is now an increased
awareness of the presence of true marine Gram-positive bacteria, with a large number
being isolated from marine sediments. Recently, Gontang et al., (2007) isolated 1,624
diverse Gram-positive bacteria spanning 22 families with 66% belonging to the class
Actinobacteria and the remaining 34% being members of the class Bacilli. Gram-
positive bacteria of the genus Bacillus have been reported in another study where B.
firmus and B. mojavensis were isolated from the marine environment (Gontang et al.,
2007; Ivanova et al., 1999; Ortega-Morales et al., 2008). Furthermore, members of
the genus are known to produce bioactive lipopeptides that are responsible for the
antibacterial activity observed (Ortega-Morales et al., 2008). This study has
highlighted anti-diatom characteristics within Bacillus, which has not been reported
previously. The mode of inhibition remains to be explored.
Chapter 2: Inhibitory activity of epiphytic bacteria isolated from Ulva
Inhibition of primary colonizers by marine surface-associated bacteria 32
2.5 Conclusion
This chapter highlights the presence of surface associated bacteria on Ulva that may
be responsible for the algae remaining unfouled in an environment prone to
biofouling. Both antibacterial and anti-diatom activities are common characteristics of
the epiphytic bacteria, with anti-diatom activity being a more widely prevalent
feature. The epiphytic anti-fouling bacterial groups identified include the genera
Shewanella, Vibrio, Bacillus and Pseudoalteromonas. The study further highlights
anti-diatom activity in Bacillus and Vibrio, groups where such action has not
previously been recognised. The close association between Pseudoalteromonas and
algal surfaces has gained a lot of attention recently. This has mainly been due to its
significant antifouling properties and success as surface colonizers. This study also
suggests a close affiliation between Pseudoalteromonas and Ulva since the strains
isolated from the algae displayed both antibacterial and anti-diatom properties.
The microfloral similarity on Ulva isolated from temperate and tropical regions is
highlighted. It is evident that Ulva supports growth of many epiphytic bacteria that
have potential as antifoulants. The abundance of Ulva, combined with warm tropical
conditions may support high bacterial diversity, leading to the discovery of novel
antifoulants. Together with advances in studies of microbial mediated defence
systems, its application will be highly beneficial for the development of antifoulants.
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 33
Chapter 3: Anti-diatom properties of Pseudoalteromonas
and Roseobacter strains
3.1 Introduction
Diatoms, like bacteria are primary colonizers of marine surfaces. Upon adhesion,
through their characteristic secretion of adhesive mucilage, diatoms play an important
role in early film formation. As the biofilm grows, adhesive exudates are released,
trapping additional particles and microorganisms, progressively leading to the
formation of a mature biofilm community (Silva-Aciares and Riquelme, 2007).
Once mature biofilms have formed on vessels, they are difficult to remove. The
development of silicone-fouling release coatings have decreased the adhesion strength
of attached organisms, which are removed as the vessel moves through water.
Although macroalgae and some hard foulers such as barnacles detach relatively
easily, diatom slimes, oysters and tubeworms are attached tenaciously and are not
easily removed, even at high speed (Callow and Callow, 2002). Due to the need for
more efficient diatom control measures researchers are now exploring natural
products for more effective alternatives (Silva-Aciares and Riquelme, 2007).
Living surfaces in the marine environment have developed efficient means of keeping
their surface free of diatoms. Dobretsov et al. (2005) assessed the settlement response
of diatoms to crude extracts of several sponge species from Hong Kong waters.
Experiments showed that 6 out of 7 sponge extracts inhibited growth and caused
mortality of the pennate diatom Nitzschia paleacea at tissue level concentration.
Similarly, a study explored the anti-diatom strategy of the blue mussel, Mytilus edulis�
(Bers et al., 2006). It was found that attachment of the benthic diatom Amphora
coffeaeformis was significantly reduced by dichloromethane extracts, whereas ethyl
acetate and diethyl ether fractions slowed diatom growth. These results provide
evidence that living surfaces in the marine environment may moderate surface
colonization of diatoms.
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 34
Pseudoalteromonas tunicata and Ph. gallaeciensis are regarded as model epiphytic
bacteria living in close association with marine algae. Both species are often isolated
from the surface of Ulva spp. and are known specifically to prevent the settlement of
common fouling organisms (Bowman, 2007; Brinkhoff et al., 2008). With the success
of P. tunicata and Ph. gallaeciensis as surface colonisers, it is predicted that other
members of these genera may also express antifouling activities. Additionally, anti-
diatom activity is a characteristic largely unexplored in Pseudoalteromonas and
Roseobacter spp. Such inhibitory activities may involve novel bioactive compounds.
The study aimed to explore and compare the prevalence of anti-diatom activity across
Pseudoalteromonas and Roseobacter spp. Since relatively little is known about the
defence strategies of epiphytic bacteria against diatoms, the study further aimed to
provide an insight into the mechanism. Information on gene identity and the
transposon Tn10 were used as tools to manipulate the genome of the model epibiont,
P. tunicata. Finally, a hypothetical model for the expression of anti-diatom activity in
P. tunicata was proposed.
3.2 Materials and methods
3.2.1 Screening Pseudoalteromonas and Roseobacter strains for anti-diatom
activity
Eight Pseudoalteromonas species strains and sixteen Roseobacter clade strain
members (Pseudoalteromonas aurantia, Pseudoalteromonas citrea,
Pseudoalteromonas piscicida, Pseudoalteromonas undina, Pseudoalteromonas ulvae,
Pseudoalteromonas haloplanktis, Pseudoalteromonas nigrifaciens,
Pseudoalteromonas tunicata, Rhodobacter sphaeroides 2.4.1, Rhodobacter
sphaeroides 17025, Rhodobacter sphaeroides 17029, Roseovarius nubinhibens ISM,
Sulfitobacter sp. EE-36, Roseovarius nubinhibens ISM, Sulfitobacter sp. NAS-14.1,
Sagittula stellata E-37, Silicibacter pomeroyi DSS-3, Dinoroseobacter shibae DFL
12, Maricaulis maris MCS10, Jannaschia sp. CCS1, Roseobacter sp. CCS2, Ruegeria
R11, Phaeobacter gallaciensis sp. 2.10 and Phaeobacter gallaciensis BS107) were
obtained from the culture collection at Centre for Marine Bio-innovation, University
of New South Wales, Australia. To screen for anti-diatom properties, the previously
described anti-diatom bioassay (section 2.2.3) was used.
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 35
3.2.2 Analysis of anti-diatom strategy of P. tunicata
Transposons are discrete DNA segments that can repeatedly insert at sites in a
genome and are therefore useful tools for genetic manipulation. In transposon
mutagenesis, random insertions occur within a specific gene and result in the loss of
function of that gene. One such system is a modified version of the transposon Tn10
known as mini-Tn10 (Herrero et al., 1990). This transposon carries a kanamycin-
resistance marker that allows for easy selection of mutants. In addition, the
transposase gene is outside of the mobile element, which allows for a stable insertion
because of the loss of the transposase gene during the transfer. A transposon mutant
library was created for P. tunicata. The library was screened for mutants lacking in
anti-diatom activity and genetic analysis of transposon insertion sites in mutants were
used to identify the affected genes.
3.2.2.1 Transposon mutagenesis
The transposon mutagenesis protocol established by James (1998) with modifications
was used to generate non anti-diatom mutants of P. tunicata. Overnight cultures of
both donor E. coli Sm 10 (containing pLOF mini-Tn 10 system) and the streptomycin
resistant recipient P. tunicata (SmR) were prepared. The E. coli strain was grown
with shaking at 37°C in LB10 medium (Appendix I) containing 85 μg/ml kanamycin
and 100 μg/ml ampicillin. The P. tunicata strain was grown with shaking at room
temperature in marine broth containing 200 μg/ml streptomycin.
The overnight cultures were washed twice to remove residual antibiotics. This was
done by spinning the cultures at 5400 × g for 2 min, then resuspending in fresh media
lacking antibiotics. After washing, the cells were resuspended in 1 volume of sterile
10 mM magnesium sulphate and gently mixed. To allow conjugation, a sterile 0.22
μm (2.5 cm diameter) membrane filter was placed onto LB15 agar plate (Appendix I)
containing 0.3 mM isopropyl-ß-D-thiogalactoside (IPTG). Donor and recipient
cultures were mixed on the membrane filter in a volume ratio of 1:3 (50 μl E. coli +
150 μl P. tunicata) and incubated for 4 hr at 30°C. Following incubation, cells were
removed from filters by gently rolling it up and placing into microcentifuge tubes
containing 1 ml marine broth and vortexed for 1 min. A 100 μl aliquot of the cell
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 36
suspension was plated onto marine agar (Difco marine broth solidified with 1.5%
agar) containing 85 μg/ml kanamycin and 200 μg/ml streptomycin to select for
recipient P. tunicata strains carrying the mini-Tn10 transposon. Plates were incubated
for 48 hr at 30°C. Colonies were transferred from agar plates to 96-well plates
containing 150 μl of marine broth containing 85 μg/ml kanamycin and 200 μg/ml
streptomycin. Plates were incubated with shaking at 30°C for 48 hr. A 65 μl aliquot of
glycerol was added to each well after the incubation period and plates stored at -80°C.
3.2.2.2 Screening for P. tunicata mutants lacking anti-diatom property
Screening for mutant phenotype was performed on 12 inch square agar plates. A 2 ml
aliquot of diatom culture was spread plated onto each plate. An ethanol sterilized 96-
pin replicator was used to transfer mutants from 96-well plates to the agar surface.
Plates were incubated inverted at 20°C in a photoperiod of 16 hr light: 8 hr dark.
Light was provided both from above and below the plates. Growth was monitored
over 5 days. Loss of anti-diatom activity was inferred if a mutant failed to produce an
inhibition zone. Plates inoculated with P. tunicata wild type served as controls.
Confirmatory tests were performed on mutant strains by re-testing for the loss of anti-
diatom activity as described above.
3.2.2.3 Growth rates of mutants
A comparison of the growth rates of transposon mutants and wild-type P. tunicata
was performed. Strains were grown in 500 ml conical flasks containing 200 ml of
growth media. The wild type P. tunicata was grown in marine broth whereas the non
anti-diatom transposon mutants, DM1, DM2, DM3 and DM4 were grown in marine
broth containing 85 μg/ml kanamycin and 200 μg/ml streptomycin. A 2 ml aliquot of
an overnight culture was inoculated into an appropriate flask and incubated shaking at
23°C. Growth was monitored by absorbance readings at 610 nm over a 24 hr period.
The experiment was carried out in duplicate and mean absorbance values were used to
plot the growth curve of tested strains.
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 37
3.2.2.4 Genomic DNA extraction of non anti-diatom mutants
Genomic DNA was extracted from mutant cultures using the XS-buffer method
(Tillett and Neilan, 2000), outlined in section 2.2.4.1. The extracted DNA was
visualized by electrophoresis on 1% (w/v) agarose gel using �-DNA digested with
EcoRI/HindIII molecular weight marker for size and concentration estimation.
3.2.2.5 Generation of adaptor ligated DNA for panhandle PCR
A suppression PCR (Siebert et al., 1995) method termed pan-handle PCR can be used
to walk from a known region into an unknown region in genomic DNA. The DNA
sequence of the mini-Tn10 transposon is known. Hence, it is possible to use the
panhandle-PCR method to obtain sequence information for the genes disrupted by the
transposon. Due to the presence of inverted terminal repeats in adaptor molecules,
PCR amplification of fragments with adaptor sequence at both ends will result in the
ends of individual DNA strands forming “panhandle” structures following every
denaturation step. Since these structures are more stable than the primer-template
hybrid, exponential amplification is suppressed (Siebert et al., 1995). In contrast, PCR
products formed by gene-specific primer and adaptor primer combinations cannot
form panhandle structures, allowing PCR amplification to continue.
Genomic DNA extracted from mutant cultures was used for restriction digestion and
ligation of adaptor molecules in a one step process. Each reaction mixture contained 1
μg of genomic DNA, 10 pmol/μl adaptor 1 (Appendix II), 10 pmol/μl adaptor 2
(Appendix II), 20 mM ATP, 2.5 units of T4 ligase, 0.5 units of blunt-end restriction
enzyme (various, see Table 3.1), 1 × respective restriction enzyme buffer and
deionised water to give a final reaction volume of 20 μl. Reactions were incubated at
20°C for 16 hr, after which the reaction was deactivated by heating to 68°C for 10
min.
The DNA was then precipitated using ethanol. Briefly, a 1/10th volume of 3 M
sodium acetate (pH 5.2) was added and mixed well. Exactly 2.5 volumes of ice-cold
absolute ethanol was then added and again mixed well. Tubes were chilled at -20°C
for 60 min. After incubation, DNA was pelleted by centrifugation at 21 000 × g and
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 38
4°C for 15 min. The supernatant was discarded and the pellet was washed in 70 %
(v/v) ethanol to remove salt. The tubes were inverted to dry the pellet, following
which DNA was resuspended in 50 μl of sterile deionised water. This solution served
as the template DNA for the PCR reactions described below.
Table 3.1: Restriction enzymes used for panhandle PCR
Restriction enzyme1 Recognition sequence
DraI TTT↓AAA
EcoRV GAT↓ATC
HincII GT(T,C) ↓(A,G)AC
HpaI GTT↓AAC
PvuII CAG↓CTG
RsaI GT↓AC
ScaI ACT↓ACT
SspI AAT↓ATT
XmnI GAANN↓NNTTC
1All enzymes were purchased either from BioLabs, Promega or Roche
3.2.2.6 Panhandle PCR
PCR was performed in 20 μl reaction volumes using 1 μl of DNA solution (as
described above), 10 mM dNTPs, 10 pmol of adaptor primer 1 (Appendix II), 10
pmol of sequence specific primer (Tn10C or Tn10D, Appendix II), 1 × Taq buffer, 2.5
mM MgCl2 and 0.05 unit of Taq polymerase added after a hot start (95°C for 2 min).
The cycle parameters were denaturion at 95°C for 30 sec and annealing/extension at
65°C for 7 min for 25 cycles. A final extension was performed at 65°C for 1 min and
samples were held at 4°C.
PCR product concentration was estimated by agarose gel electrophoresis as described
in section 2.2.4.2. Single band products were purified using QIAquick PCR
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 39
Purification Kit as per the manufacturer’s instructions. When more than one band was
present, the band of interest was excised and DNA extracted from the gel slice using
Invitrogen Quick Gel Extraction Kit following the manufacturer’s instructions. The
purified product was examined by visualizing on agarose gel once again.
3.2.2.7 Sequencing
The purified PCR products were sequenced independently using the corresponding
transposon-specific and adaptor primers. Reaction mixtures contained 15-20 pmol of
either of Tn10C, Tn10D, AP1 or AP2 primers (Appendix II), 50-100 ng of DNA
template, 5 × CSA sequencing buffer, 1 unit of BigDyeTM terminator cycle
sequencing reaction mix v.3.1 (Applied Biosystems) and sterile deionised water in a
final volume of 20 μl. Cycle sequencing was conducted using the following
thermoprofile: 94°C for 10 sec, 50°C for 5 sec and extension at 60°C for 4 min in 99
cycles. Extension products were purified by ethanol precipitation as described in
section 2.2.4.4. Separation of sequencing products was performed on an ABI 3730
DNA sequencing system at the Automated Sequencing Facility, UNSW. Sequences
obtained were compared to protein sequences available in the NCBI BLAST 2.0
(Altschul et al. 1990) and IMG 2.41 (Markowitz et al., 2008) databases in order to
identify genes disrupted by the transposon.
3.3 Results
3.3.1 Growth inhibition of diatoms
All Pseudoalteromonas strains tested showed some degree of diatom growth
inhibition (Figure 3.1). Pseudoalteromonas aurantia, P. undina and P. haloplanktis
were the most effective while P. citrea and P. ulvae were the least inhibitory.
Additionally, replicated assay plates showed varying sizes of growth inhibiton zones
produced by P. nigrifaciens. The activity of Roseobacter strains against growth of C.
fusiformis is illustrated in Figure 3.2. Approximately 44% of the Roseobacter clade
species tested displayed anti-diatom activity. Jannaschia sp. CCS1 and Phaeobacter
gallaeciensis 2.10 were the most effective, with replicated plates showing variation in
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 40
the level of activity. Nine strains of the Roseobacter clade did not inhibit diatom
growth.
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Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 42
3.3.2 Mutants lacking in anti-diatom activity
Using mini-Tn10 and the suicide vector pLOF for delivery (Way et al., 1984),
transposon mutants lacking the ability to inhibit diatom growth were successfully
generated in P. tunicata. The transposon bank consisted of approximately 1000
transconjugants. After screening it was found that 4% of the transconjugants had lost
activity. Four of the mutants (designated DM1, DM2, DM3 and DM4) were randomly
selected for re-testing. Of these, 3 were used for further genotypic analysis. Figure 3.3
illustrates the presence of a zone of growth inhibition when wild type P. tunicata was
tested against C. fusiformis and its absence when mutants of P. tunicata were used.
D2 Wild Type DM1 DM2
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Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 43
3.3.3 Growth curve of wild type and mutants of P. tunicata
To ensure that the loss of anti-diatom activity was not due to a mutation in an
essential pathway that would lead to decreased cell activity and growth, an overnight
growth experiment was performed. The wild type P. tunicata and the transposon
generated anti-diatom mutants showed no significant difference in general growth
pattern or rate. Cells entered logarithmic growth phase after approximately 2 hr and
reached stationary phase after approximately 22 hr. A graph of optical density versus
time is shown in Figure 3.4.
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3.3.4 Panhandle PCR and DNA sequencing
Using panhandle PCR, the sites within the P. tunicata genome that had been
disrupted by insertion of the mini-Tn10 transposon were amplified (Figure 3.5).
Amplified regions were further used for sequencing to determine the transposon
insertion sites.
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 44
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3.3.5 Genotype characterization of the non anti-diatom mutants
The genomic DNA regions flanking the transposon insertion sites in each of the three
mutants were analysed by sequencing. Sequencing of the 3 mutants (DM1, DM2 and
DM3) indicated different transposon insertion sites. Descriptions of each of the
insertion sites are as follows:
3.3.5.1 DNA regions flanking the transposon insertion site in DM1
Sequencing results of the analysis of DM1 showed that the transposon had inserted
into a gene, IMG locus tag PTD2_12754, with homology to a cation/multidrug efflux
pump, AcrB/AcrD/AcrF family protein. The insertion had occurred at position 227 of
the 3075 bp open reading frame (ORF) (Figure 9.1, Appendix IV). A schematic
representation of the position of the cation/multidrug efflux pump gene within the P.
tunicata genome is shown in Figure 3.6.
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 45
PTD2_12754
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In mutant DM2, the two ORFs affected were IMG locus tags PTD2_01386
(homology to a beta-hexosaminidase) and PTD2_01391 (homology to a RTX toxin
and related Ca2+ binding protein). The gene positions are schematically represented in
Figure 3.7. The sequence obtained indicated that the transposon inserted at the end of
PTD2_01386 (position 2248 in the 2280 bp ORF), extended into the intergenic region
and partially into locus PTD2_01391 (Figure 9.2, Appendix IV).
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Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 46
3.3.5.3 DNA regions flanking the transposon insertion site in DM3
Sequence analysis of DM3 showed that the transposon had inserted into a 702 bp
ORF (Figure 9.3, Appendix IV), IMG locus tag PTD2_02946, a protein with
homology to the HemeO protein family. PTD2_02946 is clustered with several other
ORFs including a long chain fatty acid (LCFA)-coA ligase and a short chain alcohol
dehydrogenase-like protein. A schematic representation of the position of
PTD2_02946 is provided in Figure 3.8.
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3.4 Discussion
3.4.1 Anti-diatom activity of Psedoalteromonas spp. and Roseobacter clade
Since all the Pseudoalteromonas strains tested inhibited diatom growth, it is obvious
that this charcteristic is prevalent within the genus. Pseudoalteromonas aurantia, P.
undina and P. haloplanktis were the most active against growth of C. fusiformis
(Figure 3.1). Previously, P. aurantia has been isolated from the surface of U.
australis and shown to produce unknown compounds that inhibit settlement of
fouling organisms (Gauthier and Breittmayer, 1979; Bowman, 2007). Additionally, P.
haloplanktis produces diketopiperazines, a probiotic beneficial to shellfish. Currently
there are no reports of bioactive compounds from P. undina (Bowman, 2007).
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 47
During a study conducted to observe the range of antifouling activities expressed by
Pseudoalteromonas spp., members of the genus produced a variety of bioactive
compounds (Holmstrom et al., 2002). Most strains inhibited bacterial and fungal
growth, algal spore germination and invertebrate larvae settlement. However, P.
nigrifaciens displayed negligible activity in most bioassays. Interestingly, in this
study P. nigrifaciens inhibited the growth of C. fusiformis. The different patterns of
diatom growth inhibition by Pseudoalteromonas strains suggest diversity within the
genus. The prevalence of anti-diatom activity may be an adaptation that allows
Pseudoalteromonas to colonize a wide range of habitats.
Strains of the Roseobacter clade tested for activity against the growth of C. fusiformis
also produced varying results. The greatest diatom growth inhibition was caused by
Jannaschia sp. CCS1, followed by Phaeobacter gallaeciensis 2.10 and
Dinoroseobacter shibae DFL 12 (Figure 3.2). Although anti-diatom activity by
members of the Roseobacter clade has not been reported previously, their
antibacterial activity has been investigated in several studies (Brinkhoff et al., 2004;
Bruhn et al., 2005; Ruiz-Ponte et al., 1998). The latter characteristic is an advantage
that may contribute to the dominance of the clade in alga-associated bacterial
communities. There may be different reasons for variation in bioactive compound
production. Certainly some strains may lack the ability to produce bioactive
compounds. For example, Ph. strain 27-4 only produces antibiotic when grown in
liquid nutrient medium under static conditions, which also facilitates rosette and
biofilm formation (Bruhn et al., 2006; Bruhn et al., 2005). Such results suggest that
culture conditions influence the production of antibacterial compounds.
Approximately half (56%) of the Roseobacter strains tested did not inhibit diatom
growth. It has been suggested that the differing physiological characteristics reflect
adaptation to the diverse ecological niches that Roseobacter occupies (Brinkhoff et
al., 2008). The lack of activity against diatoms may therefore indicate that anti-
diatom activity is not conferring a specific advantage. Members of the Roseobacter
clade are found in temperate as well as polar oceans (Brinkhoff, et al., 2008) and
dominate among marine alga-associated bacteria (Alavi et al., 2001; Buchan et al.,
2005; Gonzalez et al., 2000). It is reported that 1 in 10 bacterial cells is a member of
the Roseobacter group (Giovannoni and Rappe, 2000). Since the first description of
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 48
Roseobacter sp. in 1991, 38 affiliated and validated genera have been described
(Brinkhoff, et al., 2008). In comparison, the Pseudoalteromonas group is smaller with
as few as 35 species and 2 sub-species known to date
(http://www.bacterio.cict.fr/p/pseudoalteromonas.html). As the members of the
Roseobacter clade tested were only a small representation of the actual group,
comparison of the prevalence of anti-diatom activity to the the much smaller
Pseudoalteromonas group may be biased. Additionally, these results may suggest that
the defence mechanisms of the two groups of bacteria differ. In recent years,
members of Roseobacter have gained recognition for their antifouling properties
(Brinkhoff, et al., 2008; Rao et al., 2006). In particular, Ph. gallaeciensis is known to
be a more competitive biofilm-forming bacterium than P. tunicata (Rao et al., 2006).
With such strong anti-diatom properties and competitive biofilm-forming
characteristics, this species of Phaeobacter is worth further investigating for its
potential in preventing biofouling.
3.4.2 Analysis of transposon insertion sites within the P. tunicata genome
To study the anti-diatom strategy of P. tunicata, transposon insertion sites in non anti-
diatom mutants were analysed. In the first mutant, DM1, the transposon had inserted
into a gene homologous to the cation/multidrug efflux pump (Figure 3.6). The
cation/multidrug efflux pump (AcrB/AcrD/AcrF family protein) is an extremely
conserved gene across many phyla. The protein is synonymous to acriflavin (a
common tropical antiseptic) resistance protein in Pseudoalteromonas atlantica T6c
(66% identity). In Escherichia coli, the AcrB genes encode a multi-drug efflux
system, believed to protect the bacterium against hydrophobic inhibitors (Ma et al.,
1993). The system is energized by proton-motive force and shows the widest
substrate specificity amongst known multidrug pumps, including antibiotics,
disinfectants, dyes, detergents and solvents.
ABC transporters are generally involved in transporting ions, carbohydrates, amino
acids, antibiotics, polysaccharides and proteins (Saurin et al., 1999). ABC importers
in particular, are involved in transporting ferri-siderophore complexes across the
periplasmic space and cytoplasmic membrane back into the cells (Andrews et al.,
2003). Whether an ABC system imports or exports molecule depends upon the
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 49
presence or absence of a periplasmic binding protein associated to the coding
sequences for the ABC and transmembrane domains (Linton and Higgins, 1998).
The ABC-transporters of P. tunicata have been suggested to be involved in iron
transport (Evans et al., 2007). Analysis of the conserved domains of AcrB to
determine protein function suggests a wide range of roles. This includes defence and
transport mechanisms with a weak homology to SecD. The membrane protein SecD
is a preprotein translocase subunit which is involved in intracellular trafficking and
secretion. It may be speculated that the cation/multidrug efflux pump disrupted in
DM1 is involved either in the secretion of molecules or putative toxins responsible
for the anti-diatom property of P. tunicata.
In mutant DM2 two ORFs are affected by transposon insertion (Figure 3.7). The
transposon inserted at the end of a beta-hexosaminidase homologue that in
Pseudoalteromonas sp. strain S91 is involved in chitin degradation (Techkarnjanaruk
and Goodman, 1999). Chitin is an important component of diatom cells. A study
investigated the effects of two commercial chitin synthesis inhibitors, dimilin and
polyoxin D, on chitin fiber formation and cell sedimentation in the diatoms
Thalassiosira fluviatilis and Cyclotella cryptica (Morin et al., 1986). While dimilin
treated diatoms were indistinguishable from controls, the polyoxin D treated cells of
both diatom species completely lacked the characteristic chitin fibers. The polyoxin D
cultures were also characterized by significantly lower population densities, increased
sedimentation rates and strong tendency to clump in comparison to control and
dimilin treatments (Morin et al., 1986). One function of chitin is in the formation of
spines for diatom cell buoyancy. When the spines are removed by physical shearing
or digestion by chitinase, the otherwise intact diatom cells lose their buoyancy,
settling 1.7 times faster (Walsby and Xypolyta, 1977; Smucker, 1991). These results
highlight the importance of chitin fiber formation in diatoms and suggest the likely
impact of chitin-degrading enzymes (such as beta-hexosaminidase) produced by P.
tunicata on diatoms.
To test whether a disruption at the beta-hexosaminidase gene homologue is
responsible for loss of production of a chitin degrading enzyme further studies are
required. An experiment of the mutant’s growth on media with chitin as the sole
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 50
carbon source is suggested. Growth could be monitored by measuring optical density
over a period of 48 hr. A standard logarithmic (S-shaped) graph would indicate the
mutant’s ability to degrade chitin whereas decreased growth would indicate a
disruption that results in the loss of production of the chitin-degrading enzyme.
Located downstream of the transposon insertion site is a RTX toxin-like gene (Figure
3.7). RTX toxins are pore-forming, soluble, secreted proteins produced by a broad
range of pathogenic Gram-negative bacteria. In vitro, these most often exhibit
cytotoxic and hemolytic activities. They are particularly common in the
Pasteurellaceae which are disease causing in animals and humans (Joachim and Peter,
2002). The RTX gene cluster has also been identified in Vibrio cholerae, where it
produces proteins with haemolytic activity but also has roles in biofilm formation and
cell-cell adherence (Chatterjee et al., 2008; Lin et al., 1999). Although the function of
the RTX toxin-like genes in P. tunicata is still unknown, since it is a
Gammaproteobacteria like Vibrio, it seems likely that there would be some degree of
functional similarity between these two bacteria. This is supported by the presence of
both cadherin/sarcoglycan-homologous domains and a secretory signal peptide in the
P. tunicata (PTD2_01391) gene. These suggest a secreted protein with roles in
adhesion or cell wall stabilisation. Functional similarity of Vibrio and
Pseudoalteromonas proteins has been noted previously (Egan et al., 2002a).
The sequence obtained through Panhandle PCR and sequencing overlapped mostly in
gene PTD2_01391 (homology to RTX toxin). It is unclear if the RTX toxin gene was
disrupted which led to any change in anti-diatom activity. However, it may also be
that the intergenic region upstream of the RTX toxin gene contains regulatory
regions, the disruption of which affected the expression of RTX toxin (or other gene)
leading to a loss in anti-diatom property. Research has shown that the intergenic
region between the divergently transcribed niiA and niaD genes of Aspergillus
nidulans contains multiple NirA binding sites, which act bidirectionally (Punt et al.,
1995). Apparently, the insertion of an unrelated upstream activating sequence into the
intergenic region strongly affected the expression of both genes, irrespective of the
orientation in which the element was inserted. Also, located downstream of the RTX
toxin is PTD2_ 01396 (Figure 3.7), which is a hypothetical protein, the function of
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 51
which is not yet known. However, analysis of the conserved domains predicts the
protein to be a peptidase or a periplasmic protease.
Located upstream of PTD2_01386, are two Ton-B receptor proteins (PTD2_01376
and PTD2_01381) with roles in iron transport. Faraldo-Gomez and Sansom (2003)
also suggest TonB-dependent receptors to be responsible for the transport of large
extracellular molecules, such as vitamin B12 and iron carriers (siderophores) into the
bacterial cells. The TonB proteins in E. coli interact with outer membrane receptor
proteins that bind and take up specific substrates into the periplasmic space
(Chimento et al., 2003). In the absence of TonB, the receptors bind their substrates
but do not carry out active transport (Koebnik, 2005). The TonB complex senses
signals from outside the bacterial cell and transmits them via two membranes into the
cytoplasm, leading to transcriptional activation of target genes.
In P. tunicata, gene expression of proteins involved in iron acquisition and uptake,
including TonB are controlled by WmpR (a ToxR-like regulator, that also controls
expression of bioactive compounds, type IV pili and biofilm formation; Stelzer et al.,
2006). Recent work by Evans et al. (2007) links iron transport by TonB receptors to a
type-II secretion pathway. A disruption of the type-II secretion machinery in P.
tunicata (wmpD- mutant) results in the loss of pigment production and loss of
bioactive compounds against all target organisms. In addition, the upregulation of
TonB system biopolymer-transport proteins in the wmpD- mutant suggests a role in
transport and acquisition of iron. It has thus been suggested that the type-II secretion
pathway may be responsible for the transport of extracellular enzymes that obtain
precursor molecules for pigments and other bioactive compounds.
In mutant DM3 the transposon had inserted into PTD2_02946, a hypothetical protein
with homology to the HemeO protein family (Figure 3.8). Analysis of the conserved
domains demonstrates that the protein has heme-binding capacity. Acquisition of
heme from the environment is often for the purpose of obtaining iron (Wilks, 2002).
Neisseria meningitides and Pseudomonas aeruginosa are pathogens known to utilize
the host’s heme as an iron source. These pathogens depend on heme oxygenase for
the release of iron (Ratliff et al., 2001; Zhu et al., 2000a; b). In living organisms,
including diatoms, heme biosynthesis represents an essential metabolic pathway that
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 52
provides the precursors for cytochrome prosthetic groups, photosynthetic pigments,
and vitamin B-12 (Obornik and Green, 2005).
These results imply that a mutation in PTD2_02946, may prevent iron acquisition,
which by some means impairs anti-diatom activity. It may be that P. tunicata acquires
iron from diatom heme, an interaction that disrupts an essential metabolic pathway in
diatoms. However, this remains to be studied. At this stage we can only speculate that
iron is important either indirectly (such as in the form of a precursor of a regulatory
protein) or directly for virulence against diatoms.
Analysis of the different transposon insertion sites and corresponding loss in anti-
diatom activity can be used to propose a mechanism for anti-diatom activity in P.
tunicata. Iron is suggested to be essential for the expression of anti-diatom activity.
The HemeO homologue participates in the acquisition of iron from the environment
or directly from diatoms. Type II-secretion pathway regulates the secretion of TonB,
which would be needed to bind and transport the iron. Acquired iron is then involved
either directly or indirectly in the regulation and expression of the RTX toxin-like
gene. A multidrug efflux system is involved in pumping toxic proteins out of the
bacterial cell which lead to diatom growth inhibition. This is clearly a complex
system involving a number of steps, disruption of any one leading to loss of activity.
Further study is needed to confirm this general mechanism and fill in critical
remaining details.
Chapter 3: Anti-diatom properties of Pseudoalteromonas and Roseobacter strains
Inhibition of primary colonizers by marine surface-associated bacteria 53
3.5 Conclusion
Anti-diatom activity is a characteristic feature of many Pseudoalteromonas and
members of the Roseobacter clade. These current findings emphasize the success of
these groups as marine surface colonizers and the diversity of these groups. With the
search on for more effective means of controlling biofouling, the genus
Pseudoalteromonas and the Roseobacter clade need to be studied in much greater
detail as possible sources of antifoulants.
The ability of P. tunicata to inhibit diatom growth was studied in detail by generating
transposon mutants lacking in anti-diatom activity. Four mutants were successfully
generated, of which three were further analysed. Results suggest several possible
mechanisms of expression of anti-diatom activity. Genes observed to be important in
anti-diatom activity were predicted to have functions including a cation/multidrug
efflux pump, a beta-hexosaminidase protein, a RTX toxin and a heme binding
protein. The experiments conducted in this research will form the basis of future
studies that will identify the mechanism of anti-diatom activity in P. tunicata.
Chapter 4: General discussion
Inhibition of primary colonizers by marine surface-associated bacteria 54
Chapter 4: General discussion
This thesis describes an investigation of the antifouling characteristics of marine
epiphytic bacteria, against primary surface colonizers of Ulva spp. from Fiji. As
initial colonizers, both bacteria and diatoms are crucial for the subsequent
development of a mature biofouling community. The presence of epiphytic bacteria,
which may have a role in regulating growth of bacteria and diatoms on the surface of
Ulva, along with their identification, is addressed in Chapter 2. Anti-diatom
properties of epiphytic bacteria, which remains an under-explored area in marine
ecology, is studied in Chapter 3. This final chapter outlines and discusses the major
findings presented in the thesis and suggests directions for future work.
4.1 Antifouling properties of surface-associated bacteria
Bacteria live symbiotically on algal hosts by limiting colonization of surface foulers
in exchange for space and nutrients. Specifically, epibionts regulate biofilm formation
which benefits the host by preventing the development of a mature biofouling
community. To cooperate in such symbiotic interactions, bacteria often need adaptive
responses such as the production of antifouling molecules. Such antifouling
properties confer a competitive advantage to bacteria competing for resources.
The first two aims of this thesis were to, isolate and identify epibionts of Fijian Ulva
with inhibitory properties. Both antibacterial and anti-diatom activities were found to
be common to these bacteria. Approximately 60% of the isolates inhibited the target
bacteria and 80% inhibited growth of the diatom, C. fusiformis. The level of growth
inhibition varied widely. The red pigmented, isolate U15 (deposited under GenBank
accession FJ235137) was the most effective. This observation is consistent with
previous studies that have correlated pigmentation with natural product formation in
Pseudoalteromonas spp. (Egan et al., 2002b). Other isolates with inhibitory
properties were identified as members of Shewanella, Pseudoalteromonas, Vibrio and
Bacillus. The results were correlated with previous findings of antifouling activity
within the respective genera. Interestingly, anti-diatom activity was demonstrated in
both Bacillus and Vibrio, groups where such activity has not previously been
Chapter 4: General discussion
Inhibition of primary colonizers by marine surface-associated bacteria 55
recognized. It is speculated that many epibiotic bacteria have antifouling potential but
these remain unrecognized.
The third aim of the thesis was to screen Pseudoalteromonas and Roseobacter
isolates for anti-diatom activity. Results showed that of the tested strains, all the
Pseudoalteromonas spp. and 44% of the Roseobacter strains inhibited growth of C.
fusiformis. The research highlights the prevalence of anti-diatom activity in
Pseudoalteromonas. The lower occurance of anti-diatom activity in Roseobacter may
reflect the clade’s greater ecological diversity. It may be that anti-diatom activity does
not provide specific advantages in all cases.
The study re-emphasizes the need to preserve bacterial biodiversity especially
symbiotic forms. The technology available to assess bacterial symbioses with higher
organisms is limited (Egan et al., 2008). Advances in techniques will not only assist
in exploring existing microbial diversity for novel bioactive compounds but also
contribute significantly towards the exploitation of microbial defence mechanisms.
4.2 Modelling anti-diatom mechanism in P. tunicata
The marine epiphyte, P. tunicata is a model organism for studies of surface-
associations. The bacterium is believed to exhibit the broadest range of inhibitory
activities including antibacterial, anti-fungal, anti-algal and anti-larval characteristics
(Holmstrom et al., 2002). Although the antifouling capability of P. tunicata has been
highlighted, its anti-diatom capacity has not been explored specifically.
The final aim of the study was to identify genes involved in anti-diatom activity in P.
tunicata and suggest a model describing the mode of action. Pseudoalteromonas
tunicata mutants lacking in anti-diatom activity were generated by transposon
mutagenesis. These provided some insight into the organism’s anti-diatom strategies.
Three mutants were chosen for study and DNA sequence analysis revealed
transposon insertion at three different locations in the genome. These included a gene
homologous to a cation/multidrug efflux pump, a beta-hexosaminidase gene, RTX
toxin-like gene and a member of the HemeO protein family. Sequence analysis of
DM1 showed that the transposon had disrupted a gene homologous to the
Chapter 4: General discussion
Inhibition of primary colonizers by marine surface-associated bacteria 56
cation/multidrug efflux pump protein, belonging to the AcrB/AcrD/AcrF family.
Analysis of the conserved domains of AcrB gene suggests a wide range of roles
including defence, transport mechanisms, intracellular trafficking and secretion. The
study suggests the gene may be involved in the secretion of toxin/s responsible for the
anti-diatom activity.
The two ORFs found affected by transposon insertion in mutant DM2 were
homologous to beta-hexosaminidase and a RTX toxin. Beta-hexosaminidase is a
chitin-degrading enzyme which suggests that chitin fiber formation in diatoms may
be targeted by P. tunicata. Located downstream of the beta-hexosaminidase gene is
an RTX toxin gene. The RTX gene cluster is present in a range of pathogenic Gram-
negative bacteria and exhibits cytotoxic and haemolytic activities (Joachim and Peter,
2002; Chatterjee et al., 2008; Lin et al., 1999). Conserved domain analysis of the
RTX toxin gene suggests involvement in adhesion and cell wall stabilisation or
calcium-binding capacity. The non-coding region between the genes may contain
regulatory elements, the disruption of which could affect the expression of the RTX
gene, leading to a loss in anti-diatom activity. Interestingly, located upstream of the
beta-hexasoaminidase gene are a pair of genes encoding TonB receptors, which are
involved in iron transport. Recent work by Evans et al., (2007) links iron transport by
TonB receptors to a type-II secretion pathway. Sequence analysis of this mutant
reveals a complex system, the expression of which may be regulated by iron.
In the last mutant analysed the transposon inserted into an ORF homologous to a
member of the HemeO protein family. Conserved domain analysis suggests a heme-
binding capacity. Heme is critical for iron acquisition (Wilks, 2002). In diatoms,
heme biosynthesis represents an essential metabolic pathway which provides the
precursors for cytochrome prosthetic groups, photosynthetic pigments, and vitamin
B-12 (Obornik and Green, 2005). As with results of DM2, analysis of this mutant
suggests an important role for iron in the anti-diatom strategy of P. tunicata. Iron may
be obtained from diatoms by the HemeO homologue.
Chapter 4: General discussion
Inhibition of primary colonizers by marine surface-associated bacteria 57
Based on these results a preliminary model for the expression of anti-diatom activity
is proposed (Figure 4.1). Briefly, iron is suggested to be essential for the expression
of anti-diatom activity and is obtained by the HemeO homologue. The type II-
secretion pathway likely relates to the secretion of TonB, resulting in the binding and
transport of the acquired iron. Iron is also suggested to be involved either directly or
indirectly in the expression of the RTX toxin. Finally, the multidrug efflux system
likely pumps toxins out of the bacterial cell that inhibit diatom growth.
Extracellular environment
Cell cytoplasm
TonB TonB HemeO
Type II
Acquires iron
IronIron
Iron
Iron
Beta-hexosaminidase
Intergeneic region (controls expression of neighbouring genes)
RTX toxin
Possible precursorIron
ChitinaseMultidrug efflux pump
Putative toxin/s
Diatom heme
Relates to secretion of TonB
Binds & transports iron
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Chapter 4: General discussion
Inhibition of primary colonizers by marine surface-associated bacteria 58
4.3 Future directions and implications
Ecologically, antibacterial and anti-diatom properties give epibionts a competitive
advantage over other surface colonizing microbes when competing for space and
nutrients. Additionally, bacteria with inhibitory characteristics are often able to form
symbioses with algae, providing a microbial-mediated defence system in return for
nutrition. This study has highlighted the possibility of finding novel bioactive
compounds from tropical epibionts. Future work might investigate the defence
strategies of algal epibionts against specific target organisms. With appropriate
modification, bacterial defence systems could be used as environment-friendly
controls of biofouling.
Furthermore, the results of this research may also form the basis of future studies that
explore the mechanisms of anti-diatom activity in surface-associated bacteria,
especially P. tunicata. An in-depth study would help further develop the proposed
model. The generation of knockouts in genes already identified as important may
provide further insight into the role of the respective gene in anti-diatom activity. An
improved understanding of the anti-diatom mechanisms will provide both
environmental and economic benefits, by leading to improved methods for the control
of tenacious biofilms.
References
Inhibition of primary colonizers by marine surface-associated bacteria 59
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Appendix I: Media and buffers
Inhibition of primary colonizers by marine surface-associated bacteria 78
Appendix I
Media and buffers
Luria Broth (LB) medium (per litre)
LB 10
10 g NaCl,
10 g tryptone,
5 g yeast extract
For agar plates add 15 g agar before autoclaving
LB 15
15 g NaCl,
10 g tryptone,
5 g yeast extract
For agar plates add 15 g agar before autoclaving
XS Buffer (per 50 ml)
0.5 g potassium ethyl xanthogenate
5 ml 1M Tris-HCl, pH 7.4
2 ml 0.45M EDTA, pH 8
2.5 ml 20% sodium dodecylsulfate
10 ml 4M ammonium acetate
dH2O up to 50 ml
5 × TBE Buffer (per litre)
54 g Tris base
27.5 g boric acid
20 ml 0.5M EDTA solution (pH 8.0)
Appendix I: Media and buffers
Inhibition of primary colonizers by marine surface-associated bacteria 79
F/2 Medium (Guillard and Ryther, 1962; Guillard, 1975)
To 950 ml filtered seawater add:
Quantity Compound Stock Solution Molar Concentration
in Final Medium
1 ml NaNO3 75 g/L dH20 8.83 × 10-4 M
1 ml NaH2PO4.H20 5 g/L dH20 3.63 × 10-5 M
1 ml Na2SiO3.9H2O 30 g/L dH20 1.07 × 10-4 M
1 ml f/2 trace metal solution (see instructions below) -
0.5 ml f/2 vitamin solution (see instructions below) -
Make final volume up to around 1 L with filtered seawater and autoclave without
adding f/2 vitamin solution. Allow to cool and add filter-sterilized f/2 vitamin
solution. Sterile f/2 trace metal solution may be added after autoclaving.
F/2 Trace Metal Solution (Guillard and Ryther, 1962; Guillard, 1975)
To 950 ml filtered seawater add:
Quantity Compound Stock Solution Molar Concentration
in Final Medium
3.15 g FeCl3.6H2O - 1 × 10-5 M
4.36 g Na2EDTA.2H2O - 1 × 10-5 M
1 ml CuSO4.5H2O 9.8 g/L dH2O 4 × 10-8 M
1 ml Na2MoO4.2H2O 6.3 g/L dH2O 3 × 10-8 M
1 ml ZnSO4.7H2O 22.0 g/L dH2O 8 × 10-8 M
1 ml CoCl2.6H2O 10.0 g/L dH2O 5 × 10-8 M
1 ml MnCl2.4H2O 180.0 g/L dH2O 9 × 10-7 M
Make final volume up to 1 L with dH2O and autoclave.
Appendix I: Media and buffers
Inhibition of primary colonizers by marine surface-associated bacteria 80
F/2 Vitamin Solution (Guillard and Ryther, 1962; Guillard, 1975)
To 950 ml dH2O add:
Quantity Compound Stock Solution Molar Concentration
in Final Medium
1 ml Vitamin B12
(cyanocobalamin)
1.0 g/L dH2O 1 × 10-10 M
10 ml Biotin 0.1 g/L dH2O 2 × 10-9 M
200 mg Thiamine.HCl - 3 × 10-7 M
Make final volume up to 1 L with dH2O and filter sterilize.
Appendix II: Primers
Inhibition of primary colonizers by marine surface-associated bacteria 81
Appendix II
Primers (5'- 3')
Ad1 CTA ATA CGA CTC ACT ATA GGG CTC GAG CGG CCG
CCC GGG CAG GT
Ad2 P- ACC TGC CC -NH2
Ap1 GGA TCC TAA TAC GAC TCA CTA TAG GGC
Ap2 AAT AGG GCT CGA GCG GC
F27 GAG TTT GAT CCT GGC TCA G
R1492 ACG GTT ACC TTG TTA CGA CTT
Tn10C GCT GAC TTG ACG GGA CGG CG
Tn10D CCT CGA GCA AGA CGT TTC CCG
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Appendix IV Transposon insertion sites in the P. tunicata genome
Inhibition of primary colonizers by marine surface-associated bacteria 88
Appendix IV
Gene Sequence (PTD2_12754- IMG locus tag or ZP_01132901 Genbank accession) >gi|88857803:493602-496676 Pseudoalteromonas tunicata D2 1099591001423,
whole genome shotgun sequence
493501 tgttaggttt ttttacttta atgatccaga taacaaaata gtacaaatag attagagaaa
493561 taagcctctt gtagaacgct acaagaggct ataaaggtgt attagtgttt cttgattctt
493621 agcgctaata gacatggcgt taaaatcaat gtcagcacgg ttgcaaaggc caagccaccg
493681 gccaccgctg tggataattg cacccaccat tgagtcgatg gtgctccaaa atcaatttga
493741 cgattaaaca aatctatatt gacctgtaaa accatcggca ttaaacctaa aatagtagtc
493801 accgttgtca gtaatacagg tcttaaacgc tgagcccccg ttcttaaaat agcttcttta
493861 gcttcaatcc cctgcttaca gagcacatta taagtatcta tcagcactat gttgttattt
493921 acgacaatgc cggcaagtga aatgacacca attccagaca tcacaattcc aaatggctgt
493981 tgtaaaatta atagacccaa aaacacccct acggtcgaga aaataaccgc acttaaaata
494041 agcaaagctt gatagaagct attaaattga gtcactaaaa taattcccat cacaaaaagc
494101 gccactaaaa atgcattttg taaaaaggtt tcggattcgt tttgctcttc attttcgccg
494161 cgaactttga gcttaactct agggtcgagg ccttgctctg taagctgcgc ttgtaaacga
494221 ggcaatgcca agctcagcaa ctcccccact ttcatatcag cattaacaga cacaactcta
494281 tggctgtcaa ctcggcgcac cgaatcaact ttttgcaccg cttggcgttc tacaaagtga
494341 gttattggaa tttggccgta ttgcgtatta actcgtaagg tatctaaacg acttaaatct
494401 cgcttatcaa aaggaaagcg aactcgaata tcaatttcat catctacatc atctggccga
494461 tattcaccga gttttaaacc attggtgatc atctgcacat tcgcgccgag catggcagca
494521 tcggcaccaa atcgagcagc gtcagcgcgg ttaagtttca gctgccattc aatacccggt
494581 tttgagccag tatcatcaac attcgtgaac gatccatcag cttcaatggc ttggcgaatc
494641 cgtcttgctt cttgattcag tacttcagga aacttagagc taagctctat tgataaatct
494701 ttaccgccgc cgggaccatt ttcatcttta cgtaactcaa tttcgacgcc cgcaattgtg
494761 ctagttaacg acatcacttt ggcaataatt tggtctgcag gttctcgctc atcccaatct
494821 tttaaattta gacgcaacgt acctactaaa tccttgcctc ctgttaatga ataaagcgtt
494881 ttaatacctg caacactcag cacttttgct tcgatttctt gcattatggt gtctttttca
494941 taaatagata aatcaccata ggaacgcact ttaatattaa ccccattagg ctcaacatca
495001 ggaaaaaact caacccccag cttagatacg ccatacccaa taaaaacgaa tactgaaaat
495061 acaatcgcgc cgaataaaac tttccaagga tgcctaatgg ctcggtcaag cacccgaaca
495121 tagccaccaa taaaaccatg taactgcgtt aagtcgcctt cctcagcatt aagtaattct
495181 tgtttttgcg tggctgaaag tggcttgacc ttaccaatta aactaccaat ggtcggcaca
495241 aaaataagcg ccataactaa agaggcactt aaggtggcca ttagtgtaat aggtaagtat
495301 ttcatgaact cccccatcat acccggccaa aaaattaagg gggcaaacgc tgcaagtgta
495361 gtcgctgttg aagcaataat tggccaagcc atgcgttttg cggctagaga ataggctttt
495421 ttacggtgca ttccttcgcc catcatacgg tcggcaaatt cagtcaccac aattgcgcca
495481 tccaccagca tacctaccgc cataattaag gcaaataaca ctacgatatt aactgtcatg
495541 ccaaataacg agatcactaa aatacccgtt aaaaacgatc ccggaattgc aaccccaact
495601 aaaaaggcgg cgcggctgcc caaaatagca ataattacaa ttaccactaa caatacagct
Appendix IV Transposon insertion sites in the P. tunicata genome
Inhibition of primary colonizers by marine surface-associated bacteria 89
495661 gaaagcacat tattttgtaa atcagcaagc atttgctcaa catcaagtga catatcaccg
495721 gtgtaattaa ctttgatatg atcaggccag cgcgtgcgtg tttcttcaac cacagctttg
495781 acttgtttca cagtatcgat aatattttcg ccaacccgtt ttttaacttc aagcgatacc
495841 gctaactcac cgttaatgcg agcaatcgta ttggggtctt tataagcacg gcgaataaca
495901 gcaacatcca taaaacggac aaccttatca cccacgactt tgacaggctg ttccattaca
495961 tcttgaatcg attcaaacac tgaaggaatt tttatcgcaa aacgaccttt cccggtatca
496021 agcgtacccg cagcgattaa gcgattatta ttgctaagca actggtaaat atcattttgt
496081 tttaagccgt atgaaatcat cgctaaagga tcgacttcga tttcaaccat atcctctcta
496141 tcaccaccaa tctcaacttc taatacactt gaaattgact ccaattcatc ttttaaattg
496201 cgagcaagag tcagcaaacc acgctcaggt acattgcccg ataaggttaa tgttatggta
496261 ggctgctcgt cttccattaa tacttcatgt acttcaggct cttcagattc tgaaggtaat
496321 tttgcttttg caagcgagac tttatcgcgt acatcagcaa gggcttcttt aggatccatg
496381 cccgctaaaa actcaagtgt gactgaagca tgaccttcac ttgccactgc gctcatttct
496441 tttacgcctt caatcgaccg taattcaatt tccattgggc gtacaagcaa ccgttcggca
496501 tcctcaggtg aaataccatc atgaacaatt gagacataaa taaaaggaat tgtgacatct
496561 ggattggctt ctttggggat attttggtaa gtcacccaac cggcaataag taacaaaata
496621 aatatcgata aaccagtgcg tgtatgatga atagccgcat caatcaaatt acccataatt
496681 actcctgctc attactataa acaggttcaa cttcatcacc aatgcgcaca aacccttggc
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Gene Sequence (coding sequence 233041...578021)
Appendix IV Transposon insertion sites in the P. tunicata genome
Inhibition of primary colonizers by marine surface-associated bacteria 90
>638341157.NZ_AAOH01000001 Pseudoalteromonas tunicata D2, whole genome shotgun
sequence.
233041 ataaccgagt taaaaaatcg gggttttatt atcgtcaact agggaaataa aatgtcttat
233101 caacaaaaaa aacaaccacg ttttaatcgt tcatgtcttt gcttggctat tagcagcgcg
233161 ttactttgct ttgcggcggc ggctgaacaa aatgcaccag ccgagcaagg taaaaaactg
233221 ctcgatcttg aaaaaattat cgttacaggt accacacgtc gcggccaaac caaacttgag
233281 tcttcagtgt caattaccac cttagatgca aaacaacttg aacgagagca accccttggt
233341 actgccgatt tacttgaagt cgtgcctggt ttttgggttg aagattcggg cggtgaaact
233401 aataacaatg ttgctccacg tggtcttcgt ggcggcgaag ggtttcgtta tattggcgta
233461 gaagaagatg gcttacctgt tgtatacgat ggtgtgtggg ttgattttta tcagcgtcaa
233521 gatcttagca ttcaaaacat ggaagcggta cgtggtggta cttctggttt actcaccgtc
233581 aatggccctg cggcattagt gaattttatt acccgcaaac ccgatgatat cgaagaaggc
233641 accattcgtg tatcgactgc cgattacggc atgctcaaaa ccgaactgtt ttacggcacg
233701 ccaattagcg acaattggaa aatggcggtc ggtggttttt atcgtcattc tgaaggcgtt
233761 cgagacactg agtttagtgc tgatcacggt ggccaagtgc gcctaacgtt agttcgcgaa
233821 tttgaaaaag gccagctaac gctatctgcc aagcacctca atgatcacac tactttttat
233881 gtaccaattc cattacaaga ccaacaaaat ccaaccggga tcccaggggt tgacccacaa
233941 agtggcacct tgattggcaa cgaccaacgt ttattaagct atcgcaaagc cgatggaaat
234001 tacgttacgc gcgaccttaa agatggccag catacccaat tttcaaccct tggctttaat
234061 ttagattggg agcttagtga taactggctc atgaaattgg caggacgtta ttcaaaattc
234121 gataacgaca tgtatatttt acttaacttt gataactcga ctttaatgaa tgcaaacgat
234181 cgcttagcac aacaagatgt acagggaatg ctcagccatt ttgcagatga tggcgctgtg
234241 cgagccatgt atcggtatgt gggagacgat cacataatta acgacccaag ccaacttaat
234301 ggcaatggct tagtcaccac tagttaccct ttgttttcaa gctaccaagc tgagcaattt
234361 gtaaataaag cctcgttcac ttacgaaggc gagcaaaaca atctcaccct tggctggtta
234421 tatgcttatg ttgatgccga taccctaccc gttgataaat gggaatcaca atttttaacg
234481 gaagtacgct ctaatgcccg tcgcctcgat atagttgcag tcaataacag cggtgatgtt
234541 gtgggccagc taaccgataa cggttcaaca ggttatgcgc caggctgggg ccaagccacg
234601 gcttttggta cttcaagctc acactcattt tttattaatg atgaatttca agccaccgat
234661 gatttacgcc ttgatgcggg tattcgtatt gaatggctca agttagatag cactgcatcg
234721 ggtacgcaat tcgctgtgcc aattttgggc gcctttaacg ccaatggcga tgacagcgat
234781 aacattatgg ccaataacta tgccgatatg ccatcgagta aattttataa ccaaacccgt
234841 aacgaaaccg aagccgcgtg gacagtaggg tttaattaca cttttaataa agatatggcg
234901 atgtttggcc gctatgccga cgcttttgaa atgccacgct tattaagcca tggccaaggg
234961 atccacagcg gtaaaagcgc tgactttaac gacgtggtta atttaacctt tagcgaatta
235021 ggcttacgtt attcgggtga atcaattggt acctctgcca cattatttcg taccaagttt
235081 aatgatttaa ccgagcgtaa tttcacctca agtaacggcg cagtcgccaa tcagaccata
235141 gataccatta ccgatggcgt cgagtttgaa gcggcgtggc aagcaaccga tgatttaaaa
235201 attgagctta caggtgtggt ccaagagcct aaaatgtcgg gctttgaagg tgattttaaa
235261 cattgggaaa acaaccaagt taaacgtact ccaaaaatgc aattacgcat tactcctacc
Appendix IV Transposon insertion sites in the P. tunicata genome
Inhibition of primary colonizers by marine surface-associated bacteria 91
235321 tattatttta ataatggcga tgtgtattta accatgcacc atttaggcga tcgtttttca
235381 gatggtgaga ataaatttga attacccgcc tataccacat gggatgcagg agtgaactat
235441 caattcactt caagcctgcg cttacatgtc aaagccgcta acctgaccga tgaaattggt
235501 ttaaccgagg gtaatccacg tgccattaat gaccaacaag cgggttatga atactactat
235561 gctcgcccga ttttagggcg caccattagt gcctcgctca cctttgattt ttaagcttta
235621 tttttaatat ttgttcaact tcccccttga acttacccaa aacccaacgt ctgccaacgc
235681 ttgggtttta tttttctgtt ggagttatcg atgtattata aaattttgac cagtattagc
235741 gtattggtat tttcagcttg gctttgggct gcgccgtcaa caatctctat tgtgcctgaa
235801 ccgaaacaaa cgattgtttc aaaaggtgta ttttccctaa acaatcaaac aaaaataagt
235861 tacgacagcg acaaaagcaa gccgacagca accatgtttt ggcaaactat tgcgcccgtt
235921 accggttatc aacagccaat aacacagcgc tcggttgttg gaaaaaacca cattcatttt
235981 cagcttgata gcacactgac cacgccagaa agttatcagt tgagtgtctc tgtagagcag
236041 gttcgtattc gtgctgcgga cgtagccggg ttattttatg gcatgcaatc attgttgcaa
236101 ttactcccgc cagatattta tgccaatcat cccatcaacc aattaagttg ggatattcca
236161 gccgtcgaaa ttaatgacca accacgtttt agttatcgcg gcatgcacct tgatgtcagc
236221 cgccactttt ttaatgtgga ttttattaaa agctatattg attggctggc ctttcacaaa
236281 ctaaatgtat ttcaatggca tctaaccgat gatcaaggct ggaggataga aattaagacc
236341 tatcccaagc tcactgaagt tggatcaata cgtaatcaaa cggtattggg ccacacctat
236401 gactaccaac cactttttga tacgaccgct gtaaaggggt tttacactca agcacaaatc
236461 aaggacgtcg tggcctacgc ggcagcaaga catgtgatgg tcattcctga aatcgacatc
236521 ccgggccaca gcaccgctat tttagcggct tatccagaat taggttgcag cggtaagcgc
236581 cccgtagttg aagacaactt tggcattttt gaagcggttt tatgccccac cgagcaaacg
236641 tttgccttct tacaacaggt ttatcaagaa gtcgctacgc tttttcctgc cccttatatt
236701 catgttggtg gtgatgaagt gatcaaaaaa caatggctcg caagcccttt tgtgcagcaa
236761 ctaatgcaag agcttcagct tactagcaca gaacaagtac aaagttattt tattggcaga
236821 gtcagtaata tagtcaccgc gcttggcaaa aaaatgatcg gctgggatga aatattagaa
236881 ggtggcttag cccctaatgc cttagttacc agctggcgcg gcgaagatgg cggtgttgct
236941 gcagcaacac tgggtcatca agtaataatg agcccttatc aatttgttta ttttgatgcc
237001 tatcaatccc tgtcacagcg cgaacctaaa gcaattcatg gtttaaccac cctcaaagac
237061 gtgtatttat atgagcctat acctgcgcag ctgcccgctt cacaacatca tttagtccta
237121 ggcgcacaag gggctttgtg gacggaatac ataaaaaccc cgcaacaagc tcaatacatg
237181 ctttttccac gtattgctgc ttttgctgaa ggggtttgga gccaacctgc gcagcgcaac
237241 tggtctttgt tcacgcaaaa attgccgcta ttatttgcac gctaccaagc gcaaaacatc
237301 cattatgcac tcagccattt agtgcctgat attgccatta agcaagtcaa ctcggggcaa
237361 tcacaattaa ctattgccaa ccaattagat ggccaaattc aggttaaact gacaaatgaa
237421 acactggatc atatctacag tgaaccgctt ttagtcgata gtaataaaca agtggtgagt
237481 gtcagtgctc gtttatttgc gcccaaatta ggcctctatt ctttgcccgt acaagtcagt
237541 tttgcccacc acaaagcggt aggtaaacct attaccttaa aatacccggc gcaatctgat
237601 gggctacaaa aactcaatga tggtattttt gcttttgacc agttttaccg tgcagataat
237661 ttcgctattt tttatgatag cgacttagag gccgttatcg accttgaaaa caaaacgtca
237721 tttcatcaaa tagtcatggg tattgatgcc ggccgacatc gccaattaca tccacccatt
Appendix IV Transposon insertion sites in the P. tunicata genome
Inhibition of primary colonizers by marine surface-associated bacteria 92
237781 gcaatatcag tgtgggtatc gaatgacaag caaaattggc agcgagtaac acaattaaat
237841 gcaagtgaaa taaacggacc actccttagc tttgcggtag gtaaacagat agcacgttat
237901 gtgaaagtac acgcagttaa tgccaaaaat agtaccgatc cacaaatccc aaaattgccg
237961 ctttacatcg atgaaattgc gattttttaa tgatgattac agataaaact aagtatggct
238021 gagttcaaaa acactcacat cgctagatag tttattttta attaacaagg caaataagca
238081 ataaaaaaag ggctctgtga gccctttaaa tcagttttat agttattaat tattgcggga
238141 tatattggta aatggcttta ccataataat tggtataagc gccaccaacc gacagcagag
238201 tattaccata ggcaaccgtt ttaaagtcac gtaaataata gctagtggta tcttgcacct
238261 caaccgcaaa cggattagcg ctaagcgttt tccattgcat taaatcaaaa tcaaattgca
238321 caaagttttt tgcacttaac aggtataact tattgcctgt aagtgtagtg tcataataaa
238381 caccggctgc aaaatcagga attaactctg aatttaaaac actttgtgtt gtagtatcaa
238441 attgacttaa cagtaattgc tcatcttgac gttggataac aaaaagcgca tcacctttgc
238501 taaaacaatg ttgtatttca ttcaaactct caggtaattc tgttgcttgc cagctgttgt
238561 ccactgtatt taaacgatta aggcgttgct gttgaccatt tttagaaaac gcaatgacct
238621 caccgttaaa tgaacaactc gcttgtagcg gattactaaa tggcgcaaaa gtcggcgctg
238681 caaacgttag ccaggttttt tcttgtgtat catacacttc catattagct tgcgcatttg
238741 ccccacttga acacgcctcg gtgccaccaa agagataaag ctttttatca acaagttctg
238801 cttgataata ataacgactc gattgcggag agctcagttc ttgccaatta ttttgtgcaa
238861 tatcccaata tgacaacctt ggagcgctcg gttcggcact tgcacacaac atcgcagagg
238921 caatcgcaaa gttatgtgtc actgcataca gatcatcacc ggttgactgg acacttaaat
238981 gcgaaccttc aaaacccggt aaatcaccga gtttaaccca agatactgca atcacttcaa
239041 tatcaaatgc aggtaaagca gcttcaaatt caccatctga gacacgaata acaatgccac
239101 tggttttacc tgcatgctga tttgaaggca taccactcaa taccccagtt acagtatcaa
239161 acgtcgccca atcaggttta ttgtcaatac taaaactcaa ttgctgcgaa tcaatatctg
239221 aagccgcggc agcaaaatga tacgtttcat tcgcttgcac agtagctgct ggagttcctg
239281 taattactgg cgcatcgtta acagccgcaa gggtaatatt aacttttacc gtgctacttt
239341 ctttagagcc tttttttagt ttaaagctaa aggtatcgtc accaaattgg ttaattgctg
239401 gagagtaagt taaagcagga tacacacccg tcacttgtcc aagcgtcggt tgatttaaca
239461 gttcaacaac tacagcttca tcaccatcag ggacttgatt agcactaata cctatcgtta
239521 atgggttatc ttcagtacca ttaaccgtga tttcaggttc gacttcaaaa atgctttggg
239581 caatcacatc aacattaaag gcgggtaaag cagcttctaa ttcaccgtca gagacacgaa
239641 taacaatgcc actggttgta cctgcatgct gatttgaagg cataccactt aataccccag
239701 ttacggtatc aaacgtcgcc caatcaggtt tattgtcaat actaaaactt aattgctcag
239761 aatcaatatc tgaagccgcg gcagcaaaat gatacgtttc attcgcttgc acagcagcag
239821 ctggagttcc tgtaattact ggcgcatcgt taacagccgc aagggtaata ttaactttta
239881 ccgtgctact ttctttagtg ccttttttta gtttaaagct aaaggtatcg tcaccaaatt
239941 ggtctgctac cggcacatag cttagatttg gatatacgcc cgatatctca ccaagcgtag
240001 gttgatctac taattctaaa actatagcct cagtaccagc ggggacttta ttggcattaa
240061 tgactacagc tgatgggcta tcttccttgc ctgtaaccgt cattactggc tggatctcaa
240121 atacactttg cactagggtc ggtgtgcttt ttttatcaga acccccacag ccggttaaca
240181 atacagcaga tatagctaaa cttaaaattt tgatcttcat aataaaacca cttccgatgt
Appendix IV Transposon insertion sites in the P. tunicata genome
Inhibition of primary colonizers by marine surface-associated bacteria 93
240241 gaacagaaat ttaatgtgcc ttgcgcttct catctttacc atgcaattga cgagctatga
240301 gcaacaaaag gatagaactt cattaaatac taaagctttt tcaggtacaa gaattcatgc
240361 taattcattg taaataaatg tataaaaaaa ctgcaacacc agcaattgtc taaatttatg
240421 tttgtcacct ttaccatcac caaccaactt ttttacagct aattttataa tgaactcaat
240481 tacaccacac cgcagctttt catctttata gcttcaaacg acttaaaccc tatggtgatg
240541 gcgcttttta tgtcggtttt atcggcaaaa ttggcttgct gcgtcatttg ctctatccca
240601 ttacctaagg tgtaacgcat tttagcgctg ccatgaccgt aatatctcag ctgataagca
240661 aactgatatt ttttagtatt ggcattatac atcggctctg atatccggta ttcgagcgcg
240721 caatcattgc cgaaaaaccg ccaagcggaa taattgattt gcgctttatt ttgcgaaaag
240781 gtttcttgtg gtgtgccgcg cccttgtaaa acacggtatt caatcgctga ttgcgtagcc
240841 aaaggttggg tttcttgaaa ggctaaaaac gatgtaacca gtaaatcggg ctgaagacct
240901 agtgtctgac tttgttgggg gttgacgcca ttatgaagca caaacttgcc aactggcagt
240961 gttactttga gcttatggtg cagactcact tgctcataga tatcgacttg cccagcagta
241021 ggttcaccca caacataagc ccgtttaagg tgctgtaaag cactaacaaa acgctcagcc
241081 accacccctg tttgctcgct ggttagcaca tacaccggca catgagctcg ttttttaccg
241141 gccactcttt taagtgttgt aatgatgtcg gccttttttt taccaacttt atcaatacga
241201 tataactcag taggttgttc aaataaataa cttgcggtgt acaacaagac atcagaatcc
241261 gcattttggg ggctgcggct gtggcgcaaa tcaaaaacaa atacctcagc atccgccact
241321 tggctaaaaa gggtatcaat ttgtgtttga gtgctgtgta aatcaagttc aatcagtgct
241381 atttcatcat ttacgaatgt gatttgattc gaggccgtgg tggcagctac agcatgtgaa
241441 aggtcgggct cattcgccga tacgacaatg gagggatctt gtaacaccgc ttgcacatct
241501 tgggtcagtt tggcagcaaa gtcagcgggc tgatcaaagc ctaaatactt ataagattga
241561 tattgtttgc tgaggtgcgc tgcaattcgt ttgcctactt gtgggtcact gctgcgctgt
241621 tcaatctgta acgctaaagt attgataatt tctagctggg cttcttcgct tagtaataac
241681 gatgcttgcg agtcctcgga ataggccaac gttgctacac aagctaacat cccaacaacg
241741 agtcctttac ccatctttgc agccatccat cgcactcctt tattcgccat ttgttcctat
241801 tacacatcgg taaactagaa cattaatgca gcaggctgtc agcaaaaaaa gcacgttaat
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Gene Sequence (PTD2_02946 IMG locus tag and ZP_01132126 Genbank accession)
Appendix IV Transposon insertion sites in the P. tunicata genome
Inhibition of primary colonizers by marine surface-associated bacteria 94
>gi|88857000:575410-576111 Pseudoalteromonas tunicata D2 1099591001414, whole
genome shotgun sequence
574561 aaacaaaaca agcagacaac cggctaatgt taatttttta tagaatttca tgttgggcac
574621 ctttatttgt ttgtttcatt acttgtttca taatgactag tttttttgaa atagcgttat
574681 caactaagct tggaaaaata ccattaagct tggcaaaaaa tcgctcagga aaaccaataa
574741 cagtgcgtgc aattctgcta ttgagttgtt ttactagttg ttttgccact agctcagggc
574801 tatccatgtg attgccaaga gcagtattca tagcccgttc cagcacacca ttaatttggg
574861 tatcggttgc ccttggcgca agataaagca catcaatcgg tttatcactg agttctcttt
574921 taagcgcttc agtaaaccca cgtagaccaa acttactcgc gcaataactc gcataatatg
574981 gaaaaccaat actgccaaac gcactgccaa cattaacaat tgttgcactg tctttttgtg
575041 ataattgtgc caaaaacgct tgagttaata acatcggtac caatagattc atttcaagag
575101 tttttgagat atcaaccgca ctttgatgat caaaactggc catttgattc acgccggcat
575161 tgttaataag taccgaagca ccacctaact tttgcgcttt atgtaccaaa gcatctcgcc
575221 cttctatcgt tgctaaatcg gccgtaatat agctatgttg attacccaaa cttttagaaa
575281 gttgtgccag ttttagttca ttgcggccca ccaataacaa acgataacct tgatcatgaa
575341 gtgctgcagc cattgcttgg ccaatgccac cgcttgcgcc agtcaataca cataaaggtg
575401 attttgacat cataatgaca cctcacaatc agcattgacc tgtttagttg cagttaaacc
575461 gtgaagcggg tctaagcttc gaaacatatc accatataaa tgataaaagg catttgcact
575521 tttaatgatc agttgttgct cagatgggtc tgtaatttta tccattaaac taataaagaa
575581 cttaacgtga tcttgatcta atgcaccatg ggaacgtaaa tagctaaatg ctttatttgg
575641 aagctgaaga cggttttgca cctgcgcagc ggcgttatcg gctaatgcga tactggtgcc
575701 ttcaagcaca tgcaccatgc caaaaaagca cagcggatta attctgctca cacaatcata
575761 cgcatacgat accattaatt cggtcgcaaa taatggcgtt gacttacgtg cttgttcttt
575821 atcataacca caagctgcaa tatcgtttaa tacccattct tgatggccaa gttcttcttc
575881 aatatattct gcaacttcat ttcgcagcca ttctttggat tctggtaatc gacttccaac
575941 agccattaat aaaggtgttg tatgcttaac atgatgataa gcctgctgta aaaaggcgac
576001 ataatcatca atgctaaatt gacctgcaaa acaacgttga ataatcggtg cttgtagaag
576061 atattgctgc gactgctgtg ttttttgtac tagtgtttga taaaaactca taatgactcc
576121 aaagcagaac caacaggttc agcacattgt gatttagatg cataaagggc gttaacttgg
576181 gccgcaaaat gcgtagcaat ttctgttctt tttggtcggt tgtttgcggt ataaagatta
576241 tcgatttgac tcattggtgc attgagtact tcatacgccc gtacttttgc gtaatcgggt
576301 aattgtgcat taactttatt gatggcagca ctcagattgg cctcatccat tggtttaatt
576361 ggtacaagca aagcaataca gaatggtctt tcttcaccta atacaaccgc ttggtaaaaa
576421 aggccggtcg cttgcaataa gctttcaggc cattcggggg cgatattgcg accaaagctt
576481 gaaataatca gatttttttt acgaccattg ataattaaaa agtcgtcgtt aataacagct
576541 aaatctcccg ttttgaactc tcgcgcaaac caagaatcgg gatcgttttg gtatcccaag
576601 tggcaattgc cacagacaac taattcacca tcaacttcat atacttgaca atgaggcagc
576661 actttacctg cactggcatg attacaatcc aaaggcgtat ttaggctcac caccgagcca
576721 cactccgaaa gtccatagcc ttgataaaca ggtaaaccta atctgtgggc ttcttctaat
Appendix IV Transposon insertion sites in the P. tunicata genome
Inhibition of primary colonizers by marine surface-associated bacteria 95
576781 aaatcacacg cgacttttgc accaccaaca gcgataaatt tcaacgatgt cggtgtagtc
576841 caacctgcct tgattgcatt gaccaataac agcaacagtt caggtactaa aattaaagag
576901 ttcggttcag cacggctaat attcatcaag agtttatttg gctcaaccag cttagtaccg
576961 ttaaaaccta atgcttcaag ggatacaagc gtcacagtgc caccagccaa taagggcgca
577021 tacacccctg cgatattttc taacaaaacc gaaaggggta ataaacaaag gtgttttggc
577081 gcttttaaag cgatagcatc aactaatgag tgagccacta ctgtctgatt ttcaacagat
577141 aagcacaccc cttttggtaa accggtagag ccagaagtaa aggtgacttt ttgggtacca
577201 ttaggtcgca tgccaaagtc tgattgcatt aattgtgcga taaataaagt gcggccaaag
577261 ccaacaaaca cctcactacc gacagccgaa atatcattat taatctgctc actgataaaa
577321 caatcgaccg ctgagctctc aattaaatgt ttaatttggc tttcagtaaa aaataaaggc
577381 actgagataa ttgtgatatt cgcttgttgc gcagctaaat caaacaaaat ccattcaatg
577441 caattatcga tatgtagtgc cagagtttgc acgtttaaat gagttaataa gcggctcctt
577501 acatgtacgg cttctatcag ttgttcgtaa cttaattgac attcaccatc gtctaacgca
577561 atgcgagttt caaattggct tatcgaatct atcaagctca taattgagtc acctctggca
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