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Accepted Manuscript
Optimization of Cellulase production by a brown rot fungus
Fomitopsis sp.
RCK2010 under Solid State Fermentation
Deepa Deswal, Yogender Pal Khasa, Ramesh Chander Kuhad
PII: S0960-8524(11)00374-9
DOI: 10.1016/j.biortech.2011.03.032
Reference: BITE 8265
To appear in: Bioresource Technology
Received Date: 25 January 2011
Revised Date: 10 March 2011
Accepted Date: 11 March 2011
Please cite this article as: Deswal, D., Khasa, Y.P., Kuhad,
R.C., Optimization of Cellulase production by a brown
rot fungus Fomitopsis sp. RCK2010 under Solid State
Fermentation, Bioresource Technology (2011), doi: 10.1016/
j.biortech.2011.03.032
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Optimization of Cellulase production by a brown rot fungus
Fomitopsis sp. RCK2010
under Solid State Fermentation
Deepa Deswal, Yogender Pal Khasa and Ramesh Chander Kuhad*
Lignocellulose Biotechnology Laboratory, Department of
Microbiology, University of Delhi
South Campus, Benito Juarez Road, New Delhi-110021, India
*Corresponding Author: Prof. Ramesh Chander Kuhad
Lignocellulose Biotechnology Laboratory
Dept. of Microbiology
University of Delhi South Campus
Benito Juarez Road
New Delhi-110021, India
Email: [email protected]
Tel: +91-11-24112062
Fax: +91-11-24115270
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Abstract
Culture conditions for enhanced cellulase production from a
newly isolated brown rot fungus,
Fomitopsis sp. RCK2010 were optimized under solid state
fermentation. An initial pH of 5.5
and moisture ratio of 1:3.5 (solid:liquid) were found to be
optimal for maximum enzyme
production. Of the different carbon sources tested wheat bran
gave the maximum production
of CMCase (71.526 IU/g), FPase (3.268 IU/g), and -glucosidase
(50.696 IU/g). Among the
nitrogen sources, urea caused maximum production of CMCase
(81.832 IU/g), where as
casein and soyabean meal gave the highest FPase (4.682 IU/g) and
-glucosidase (69.083
IU/g) production, respectively. Among amino acids tested
glutamic acid gave the highest
production for CMCase (84.127 IU/g); however 4-hydroxy-L-proline
stimulated maximum
FPase production (6.762 IU/g). Saccharification of pretreated
rice straw and wheat straw by
crude enzyme extract from Fomitopsis sp. RCK2010 resulted in
release of 157.160 mg/g and
214.044 mg/g of reducing sugar respectively.
Key words: Brown rot fungus, cellulase, optimization,
saccharification.
.
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Introduction
The growing concern for depleting fossil fuel requires a
transition from non-renewable carbon
sources to renewable bioresources such as lignocellulose.
Regardless of the source,
lignocellulosic materials consist of three main polymers;
cellulose, a homopolymer of glucose;
hemicellulose, a heteropolymer of pentoses and hexoses; and
lignin, an amorphous polymer of
phenyl propanoid units (Kuhad et al., 1997). Among these
cellulose fits in the role perfectly
and thus is also referred as the biological currency (Himmel et
al., 1999). Every year plants
produce about 180 billion tons of cellulose, making this
polysaccharide a huge organic carbon
reservoir on earth. The cellulose synthesis rate is estimated to
be equivalent to 70 kg per
person per day (Lutzen et al., 1983). Therefore the importance
of cellulose as a renewable
source of energy has become a subject of both, intense research
and of commercial interest.
The key step in the utilization of cellulose is its hydrolysis
into monomeric sugars and their
eventual conversion into valuable chemicals and energy (Olofsson
et al., 2010).
The enzyme, which governs the hydrolysis of cellulose, is known
as cellulase. Unlike most
of the enzymes cellulase is a complex of enzymes that work
synergistically to attack native
cellulose. Cellulase is a family of at least 3 groups of
enzymes: firstly endoglucanases (EC
3.2.1.4) which act randomly on soluble and insoluble cellulose
chains; secondly exoglucanases
(cellobiohydrolases EC 3.2.1.91) that act to liberate cellobiose
from the reducing and non-
reducing ends of cellulose chains and finally, -glucosidases (EC
3.2.1.21) which liberate
glucose from cellobiose. The cellulases give us an opportunity
to reap the tremendous benefits
of biomass utilization in an eco-friendly manner (Himmel et al.,
1999). Besides this, cellulases
have many other potential applications as well, for example,
formulation of washing powder,
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animal feed production (Han et al., 2010), textile industry,
pulp and paper industry, starch
processing, grain alcohol fermentation, malting and brewing,
extraction of fruits and vegetable
juices (Bhat, 2000). Therefore, like cellulose, a wide range of
applications have made cellulase
one of the most desirable enzyme system. An efficient cellulose
hydrolysis requires a high
enzyme loading and except recombinants, the level of cellulase
production from majority of
the microorganisms has been generally low. The requirement of
high amount of the enzyme
makes the hydrolysis process economically less favorable. In
many bioconversion strategies,
the cellulase required for biomass conversion may account for as
much as 40% of the total
process cost (Ahamed et al., 2008). Therefore large scale low
cost production of cellulase is
very important for the overall process economics for
bioconversion of lignocellulosics into
value added chemicals such as ethanol as biofuel.
A large number of microorganisms such as bacteria, actinomycetes
and fungi (Kuhad et al.,
1997; Kalogeris et al., 2003) are known to degrade cellulose.
Among fungi, soft rot and white
rot have been extensively studied while brown rots have not been
studied much. Cellulolytic
enzymes from soft rot and white rot fungi have been studied in
model organisms such as
Trichoderma viride and Phanerochaete chrysosporium respectively.
T. viride produces fairly
good amount of exoglucanases and endoglucanases but low level of
-glucosidase, which is
insufficient for effective conversion of cellulose to glucose.
However, the brown rot fungi
differ substantially from soft-rot and white rot fungi with
respect to the cellulolytic enzymes
produced and the pattern of cellulose degradation (Kuhad et al.,
1997). These fungi are
generally reported to lack the exoglucanases that can hydrolyze
crystalline cellulose (Kuhad et
al., 1997), yet they cause the most destructive type of wood
decay and are important
contributors to biomass recycling. Recently brown rot fungi such
as Fomitopsis has been
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reported to hydrolyze microcrystalline cellulose and therefore
has been studied in some
laboratories (Yoon et al., 2008).Yoon et al. (2005) have
reported the degradation of crystalline
cellulose by Fomitopsis palustris. However, to the best of our
knowledge the cellulase
production from Fomitopsis sp. has not been optimized.
Beside the fungus type, the cellulase production is also greatly
influenced by media
components, especially carbon and nitrogen sources, minerals and
physical factors such as pH,
temperature and moisture (Lynd et al., 2002). In order to obtain
maximum enzyme production,
development of a suitable medium and culture conditions is
obligatory. Solid-state
fermentation (SSF) conditions have shown to be potential for
enzyme production by the
filamentous fungi (Holker et al., 2004). The commercial
production of enzymes is carried out
through SSF for its obvious advantages over liquid cultivation
(Viniegra-Gonzalez et al.,
2003; Holker et al., 2004). The substrate used in SSF for
cellulase production is deterimental
in economizing the enzyme production process. Therefore, various
cellulosics substrates such
as sugarcane bagasse, corn stover, wheat straw, and wheat bran
have been tested by several
workers for production of cellulases.
In this paper we report the optimization of various
physiological and nutritional parameters for
cellulase production from newly isolated brown rot fungus
Fomitopsis sp. RCK2010 using
cost effective substrates under solid state fermentation
cultivation conditions. Moreover an
attempt has been made to study the application of cellulase(s)
in hydrolysis of lignocellulosic
substrates such as wheat straw and rice straw.
Materials and Methods
Raw Materials and their Pretreatment
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Lignocellulosic substrates like Wheat straw (WS), Rice straw
(RS), Wheat bran (WB), Corn
cob (CC), Corn Stover (CS), Prosopis juliflora (PJ), and Lantana
camera (LC) were obtained
locally. They were first dried and chopped into small pieces by
a chopper, then ground into
smaller particles in a hammer mill (Metrex Scientific
Instrumentation Pvt. Ltd., New Delhi,
India) and finally separated by 20 mesh sieve.
The pretreatment of both the substrates (rice straw and wheat
straw) was carried out separately
with 0.5% (w/v) H2SO4 and 2.5% NaOH at 121C for 15 min. The
pretreated residues were
washed extensively to neutral pH and dried at 60C till constant
weight.
Microorganism and culture conditions
The fungal isolate RCK2010 procured from the culture collection
of Lignocellulose
Biotechnology Laboratory, Department of Microbiology, University
of Delhi South Campus,
New Delhi, India was grown and maintained on malt extract agar
(MEA) composed of (gl-1):
malt extract, 20.0; Ca(NO3)2.4H2O, 0.5; MgSO4.7H2O, 0.5; KH2PO4,
0.5; and agar, 20.0 (pH
5.5) at 30C (Dhawan et al., 2002; Vasdev et al., 2005). The
fungal cultures were maintained
by periodical subculturing on MEA at 30C and stored at 4C.
Identification of the fungus
Isolation of Genomic DNA
Fungal isolate RCK2010 was grown in malt extract broth (MEB) as
described elsewhere
(Dhawan et al., 2002; Vasdev et al., 2005) at 30C under static
cultivation conditions for 168
h. The cultures were harvested by filtering through Whatman No.1
filter paper. The fungal
mycelium was thoroughly washed with Milli Q water and ground in
liquid nitrogen. Genomic
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DNA of fungal mycelium was isolated using method modified by
Kuhad and coworkers as
reported earlier (Kuhad et al., 2004).
Phylogenetic studies of the fungus
ITS sequence of fungal isolate RCK 2010 was amplified by PCR
using pITS-1 (5-
TCCGTAGGTGAACCTGCGG 3) and pITS-4 (5- TCCTCC
GCTTATTGATATGC-3)
primer pair. Following cycling parameters: an initial
denaturation at 94C (4 min), 35 cycles of
primer annealing at 58C (40 sec), elongation at 72C (1 min) and
denaturation at 94C (1
min). A final elongation step was allowed at 72C for 8 min. The
PCR product was eluted
using gel extraction kit (Quigen Sciences, Maryland, USA) and
was sequenced at The Centre
for Genomic Application (TCGA) Okhla, New Delhi, India. Sequence
obtained was compared
with ITS sequences available in GenBank, using Clustal W and a
dendrogram was constructed
to establish the taxonomic rank of the fungus (DNA STAR,
Madison, WI, USA).
Inoculum preparation
Each Erlenmeyer flask (250 ml) containing 50 ml of MEB was
inoculated with four mycelial
discs (0.8 cm dia each) and incubated at 30C under static
cultivation conditions for 7 days.
The mycelial mat thus obtained was homogenized with pestle and
mortar under sterile
conditions and used as primary inoculum for further
experiments.
Cellulase production under solid state fermentation
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Solid state fermentation was carried out in 250 ml Erlenmeyer
flasks, each having 5.0 g of dry
Wheat bran moistened with mineral salt solution (gl-1:(NH4)2SO4,
0.5; KH2PO4, 0.5; MgSO4,
0.5 and pH 5.5) to attain the final substrate-to-moisture ratio
of 1:3.5. The flasks were
sterilized by autoclaving at 121C (15psi), and thereafter cooled
to room temperature and
inoculated with desired volume of inoculums to obtain 0.25 g
0.013 of fungal dry mass
(0.5% w/w). The contents of the flasks were mixed well with
sterilized glass rod to distribute
the inoculum through out the substrate and incubated at 30C. The
fungal fermented wheat
bran (myco-bran) was aseptically removed from flasks after an
appropriate interval, suspended
in 50 ml citrate buffer (100 mM, pH 5.5) and shaken gently for
45 min. The extrudates were
squeezed through muslin cloth for maximizing the enzyme
extraction and centrifuged at
10,000 rpm at 4C for 10 min. The enzyme solution thus obtained
was assayed for various
cellulase activities to study their time course production.
Optimization of cellulase production
The cellulase production by the fungus was optimized following
one factor at a time (OFAT)
approach. The effect of various factors such as initial pH
(3.0-10.0), incubation temperature
(25-40C), substrate to moisture ratio (1:1-1:4), metal ions
(2mM), and different carbon and
nitrogen sources, as described in the text, was tested. In
addition effect of amino acids (0.2 %
w/w), vitamins (0.2% w/w) and surfactants (0.2% w/w) to enhance
cellulase production was
also investigated.
Application of cellulase in cellulose hydrolysis:
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Enzymatic hydrolysis of untreated and pretreated substrates
(rice straw and wheat straw) was
carried out at 2% (w/v) consistency in 50mM citrate phosphate
buffer (pH 4.8) containing
0.005% (w/v) sodium azide. The flasks were added with crude
enzyme solution equivalent to
FPase activity of 25 IU/g pretreated substrate and incubated at
50C and 150 rpm for 24 h.
Samples were withdrawn at regular intervals, centrifuged at 8000
rpm for 10 min and the
supernatant was analyzed for reducing sugars released.
Analytical methods
The total cellulase (filter paper cellulase, FPcellulase),
Carboxymethyl cellulase (CMCase)
and -glucosidase activities were determined in accordance with
the International Union of
Pure and Applied Chemistry procedures as reported by Ghose
(1987). FPcellulase (FPase)
activity was assayed by measuring the release of reducing sugars
in a reaction mixture
containing Whatman No.1 filter paper (1.0 cm x 6.0 cm 50.0 mg)
as substrate in 50mM
sodium citrate buffer (pH 4.8) at 50C, after 60 min.
Carboxymethlycellulase (CMCase)
activity was assayed by measuring the release of reducing sugars
in a reaction mixture
containing 0.5 ml of crude enzyme and 0.5 ml of 2% (w/v) of CMC
solution in 50mM sodium
citrate buffer (pH 5.5) incubated at 50C for a period of 30 min.
Reducing sugars were assayed
by dinitrosalicyclic acid (DNSA) method of Miller (1959).
-Glucosidase activity was
determined by assaying the release of p-nitrophenol (pNP) at 430
nm from a reaction mixture
containing 1 ml p-nitrophenyl glucopyranoside (pNPG) (1 mM), 1.8
ml acetate buffer and 0.2
ml suitably diluted enzyme, incubated at 50C for 30 min (Wood et
al., 1969). One unit of
enzyme activity was defined as the amount of enzyme required to
liberate 1mole of glucose
or p-nitrophenol, from the appropriate substrate, per ml per
minute under the assay conditions.
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Results and Discussion:
Identification of Fungus RCK2010:
The fungal isolate RCK 2010 was identified based on the sequence
variation present in
internal transcribing spacer (ITS) region. Sequence analysis
suggested that RCK 2010 was
phylogenetically related to members of the genus Fomitopsis,
where it showed maximum
similarity of 93% with the Fomitopsis genus (Figure 1). Based on
this sequence homology, the
fungus RCK2010 was identified as Fomitopsis and hereafter it is
named as Fomitopsis sp.
RCK2010. The sequence had been deposited in NCBI Genbank
database with accession
number: GU991381.
Time course of cellulase production:
Fomitopsis sp. RCK2010 grown under SSF started producing all the
three cellulases on day 2
of incubation. The CMCase production peaked (71.699 IU/g
substrate) on eleventh day,
whereas maximum -glucosidase (53.679 IU/g substrate) and FPase
(3.492 IU/g substrate)
production was observed on the fifteenth and sixteenth day,
respectively (Figure 2). Any
further increase in incubation did not favor any increase in the
enzyme production. The exact
comparison of cellulase production by different microorganisms
reported in literature may not
be possible because many a times different laboratories estimate
the enzyme under different
conditions. However, the comparison of cellulase production by
Fomitopsis sp. RCK2010
under SSF with ones earlier reported showed that the fungus
tested in this study produced
fairly good amount of cellulases (Table 1).
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Effect of Physiological Parameters on cellulase production
Temperature is one of the most important physical variable
affecting solid-state fermentation
(Krishna, 2005). The optimization of incubation temperature for
production of cellulases from
Fomitopsis sp. RCK2010 under SSF conditions revealed that the
enzyme production gradually
increased from 25-30C (Figure3) and maximal enzyme production of
all the three enzymes
viz. CMCase (70.784 IU/g), FPase (3.247 IU/g) and -glucosidase
(50.989 IU/g) was observed
at 30C. Any increase in temperature beyond 30C had a drastic
adverse affect on the enzyme
production. Hanif and co-workers (2004) also reported an
increase in cellulase production
from Aspergillus niger up to 30C and thereafter the production
of enzyme declined. Wang et
al. (2006) while studying the optimization of multienzyme
production by two mixed strains
Aspergillus niger F3 and Aspergillus niger F4 in solid state
fermentation also reported the
similar temperature optima.
The pH of the medium is one of the most critical environmental
parameter affecting the
mycelial growth, enzyme production and the transport of various
components across the cell
membrane (Kapoor et al, 2008). The cellulase production by
Fomitopsis sp. RCK2010 was
also tested at different pH ranging from 3.0 to 10.0. The fungus
produced maximum CMCase
(72.696 IU/g), FPase (3.307 IU/g) and -glucosidase (50.951 IU/g)
at initial medium pH 5.5
(Figure 4). Increasing the initial pH of the medium from 5.5 to
10.0 showed a significant
decrease in the production of cellulases. A loss of more than
50% in enzyme production was
observed at initial medium pH of 10.0. The decrease in initial
pH of the medium from 5.5 to
3.0 also caused a slight decrease in the CMCase and FPase
production. The optimum initial
pH for maximum fungal cellulase production has been reported to
be variable in majority of
the cases (Niranjane et al., 2007). The -glucosidase produced by
the fungus retained more
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than 90% of its optimal activity at pH ranging from 3.0 to 7.0.
Although further increase in pH
caused a decrease in enzyme production. Kalogeris and co-workers
(2003) also reported a
decrease in the -glucosidase by Thermoascus aurantiacus, when
the pH of the production
medium was shifted from acidic to alkaline.
The moisture content of the growth medium is critical variable
affecting the solid-state
fermentation. The optimal moisture content in solid-state
fermentation depends on the nature
of substrate, the requirements of microorganism and the type of
end product (Kalogeris et al.,
2003). The result of this study has shown that an increase in
the initial moisture ratio from 1:1
to 1:3.5 greatly enhanced the enzyme production (Table 2) of all
the three cellulases. The
substrate to moisture ratio of 1:3.5 resulted in maximum
production of CMCase (72.071 IU/g),
FPase (3.191IU/g), -glucosidase (66.594IU/g). However, any
further increase in moisture
level in Solid State fermentation showed lower enzyme production
which may be attributed to
particles sticking, limited gas exchange and higher
vulnerability to bacterial contamination,
while low moisture leads to reduced solubility of nutrients,
substrate swelling (Hamidi-
Esfahani et al, 2004).
Effect of nutritional parameters on cellulase production
Extracellular enzyme production depends greatly on the
composition of the medium. Various
lignocellulosic substrates were tested as carbon source for
their effect on cellulase production.
The influence of the carbon sources on cellulase production by
Fomitopsis sp. RCK2010 is
depicted in Table 3. Among the carbon sources tested, wheat bran
was found to induce
maximum production of CMCase (71.526 IU/g), FPase (3.268 IU/g)
and -glucosidase
(50.696 IU/g). It is well known that the type and composition of
the carbohydrates present in
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wheat bran are suitable for the induction of cellulases in
filamentous fungi under solid-state
fermentation (Jecu, 2000). The cellulase production by
Fomitopsis sp. RCK2010 was found to
be at low level when grown on other lignocellulosic materials
like corncob and Prosopis
juliflora. The unsuitability of the lignocellulosic substrates
to support enzyme production
under solid-state fermentation might be due to inappropriate
physical properties like particle
size, geometry and compactness of the substrate (Krishna,
2005).
Different nitrogen sources have shown variable effects on
cellulase production by Fomitopsis
sp. RCK2010 (Table 4). Among various organic nitrogen sources,
urea caused maximum
CMCase (81.832 IU/g) production, whereas casein and soyabeen
meal resulted in maximum
FPase(4.682 IU/g) and -glucosidase(69.083 IU/g) production
respectively. The inorganic
nitrogen sources did not exhibit any significant effect on
increase in enzyme production. Our
results are in agreement with the observations of Daroit et al.
(2007). However, some studies
have also shown that inorganic nitrogen source resulted in
improved enzyme production
compared to organic nitrogen source (Kalogeris et al.,
2003).
Presence of metal ions was shown to influence enzyme production
by microorganism in
culture. Various metal ions (2mM) were used as additives in the
basal medium to determine
their stimulatory or inhibitory effect on enzyme production
(Figure 5). An increase in CMCase
production was observed when the production medium was
supplemented with zinc (92.979
IU/g) and nickel ions (89.059 IU/g), while mercury (40.817 IU/g)
and calcium (41.125 IU/g)
exhibited an inhibitory effect. The addition of sodium (6.388
IU/g), manganese (6.831 IU/g)
and copper (6.795 IU/g) had a stimulatory effect on FPase
production. The fungus was
observed to produce maximum -glucosidase (98.971 IU/g) in
presence of barium ions but the
addition of potassium (41.549 IU/g), calcium (44.779 IU/g) and
ferric ions (41.903 IU/g)
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14
inhibited the -glucosidase production. According to observations
made by us, zinc and nickel
supplemeted medium enhanced the production of all the three
cellulase enzymes. These results
can be attributed to the fact that the metals might be acting as
cofactors for many enzymes
involved in intermediatory metabolism (Jellison et al.,
1997).
Among various amino acids and their analogues studied, the
maximum CMCase production
(84.127 IU/g) was observed in the presence of L-glutamic acid,
whereas, aspartic acid (79.099
IU/g), asparagine (77.844 IU/g) and L-cystine (76.799 IU/g)
comparatively brought about a
lesser increase in CMCase production (Table 5). L-methionine and
L-phenylalanine
completely inhibited CMCase production. There was a significant
increase in FPase
production on addition of 4-hydroxy-L-proline (6.762 IU/g),
glycine (6.264 IU/g) and L-
cystine (6.177 IU/g). Our observations are in accordance with
earlier reports where increase in
laccase production has been reported in presence of glycine
(Dhawan et al., 2002). Changes in
the membrane permeability in presence of glycine had been
reported due to release of
enzymes extracellularly (Dhawan et al., 2002). Addition of
L-isoleucine gave the maximum -
glucosidase production (77.546 IU/g).
The presence of vitamins usually affects the rate of
biosynthesis of many metabolites.
Ascorbic acid supplementation gave maximal FPase (5.668 IU/g)
and -glucosidase (92.251
IU/g) (Table 5). Riboflavin and biotin also exhibited a
stimulatory effect on FPase and -
glucosidase production. Biotin is well documented for playing
important role in functioning of
several physiological and metabolic enzymes including pyruvate
carboxylase and several
tricarboxylic acid cycle auxillary enzymes (Entcheva et al.,
2002). Our results are in
accordance with the earlier reports where the effect of vitamins
was studied on laccase
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15
production (Dhawan et al., 2002). Interesting to note that none
of the vitamin tested here did
not induce the CMCase production.
The use of surfactants in the production of hydrolytic enzymes
is well known (Kapoor et al.,
2008). PEG of different molecular weights were used to study
their effect on cellulase
production. It was observed that there was a gradual increase in
cellulase production with
increase in molecular weight of PEG upto 6000, which gave
maximum CMCase (79.544
IU/g), FPase (5.137 IU/g) and -glucosidase (61.502 IU/g)
production. These results are in
accordance with our previous studies, where the addition of
Tween 80 enhanced the cellulase
production by 30% (Kuhad et al., 1994). In the present study,
Triton X-100 maximally
enhanced CMCase (98.268 IU/g), FPase (6.711 IU/g) and
-glucosidase (65.361 IU/g)
production from Fomitopsis sp. RCK2010 (Table 5). Such compounds
probably increase the
permeability of the cell membrane, allowing more rapid secretion
of enzymes (Ahamed et al,
2008).
Enzymatic hydrolysis
The efficacy of crude cellulases from Fomitopsis sp. RCK2010 in
hydrolyzing the untreated
and pretreated rice straw and wheat straw was evaluated. The
time course of enzymatic
saccharification revealed that irrespective of the substrate and
pretreatment used, the release of
sugars increased with increase in the saccharification time
studied here (Figure 6). However,
the maximum sugars were released on enzymatic hydrolysis of
alkali pretreated wheat straw
(214.044 mg/g of substrate), more than from alkali pretreated
rice straw (157.160 mg/g of
substrate) after 24h (Figure 6). This higher increase of
reducing sugars in alkali pretreated
substrates may be attributed to the release of lignin moieties
during alkali treatment which in
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16
turn enhanced the accessibility of cellulose to the enzymes
(Gupta et al., 2010). While,
comparatively the lower release of sugars in acid treated
substrate may be due to the
relocalization of acid hydrolyzed lignin to the surface of
substrate (Hendriks et al., 2009).
Earlier there were several reports with commercial enzymes from
T. reesei, a soft rot fungus,
to release higher amount of glucose during enzymatic
saccharification of cellulosics, however,
the saccharification of cellulosic substrates with the enzymes
from brown rot fungi has been
comparatively lower (Table 6). The higher saccharification of
cellulosics by commercial
preparations could be because these contain different cellulases
in pure form and also because
the delignified (chlorite pretreated) substrate used in these
studies were of high cellulose
purity (~90% w/w) (Gupta et al 2011), when compared with the
hydrolysis of alkali treated
wheat straw and rice straw, the partially delignified cellulosic
substrates, with crude cellulase
from Fomitopsis sp RCK2010 (Table 6). Interestingly, the enzyme
from Fomitopsis sp.
RCK2010 has shown comparatively higher saccharification
efficiency than the enzymes from
brown rots reported earlier (Table 6). Yoon et al. (2005) have
reported a release of only 32
mg/g sugar from avicel after 43h, while Lee and coworkers (2008)
when enzymatically
hydrolyzed Pinus densiflora observed only 3.53 mg/g sugar
release.
Conclusion
Our study indicates that Fomitopsis sp. RCK2010 has good
potential in producing complete
cellulase and hydrolyzing the cellulosics into fermentable
sugars. Moreover, if the cellulase
production form this fungus is further optimized using
statistical methods such as response
surface methodology (RSM) which uses combinatorial interactions
of culture conditions, it
may result in improved production of cellulases.
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17
Acknowledgement
The authors are grateful to Council of Scientific and Industrial
Research, Government of
India, New Delhi, India, for the financial support during the
progress of this work.
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Legend to figures
Figure 1: The phylogenetic dendogram for Fomitopsis sp. RCK2010
and related fungal
strains based on ITS sequence
Figure 2: Time course of cellulase production by Fomitopsis sp.
RCK2010 under Solid state
fermentation
Figure 3: Effect of temperature on cellulase production by
Fomitopsis sp. RCK2010 under
SSF
Figure 4: Effect of pH on cellulase production by Fomitopsis sp.
RCK2010 under SSF
Figure 5: Effect of different ions on cellulase production by
Fomitopsis sp. RCK2010 under
SSF
Figure 6: Enzymatic hydrolysis profile of alkali and acid
treated rice straw and wheat straw
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23
Fomitopsis cf. meliae KYO
Fomitopsis cf. meliae 1P 1 1
Fomitopsis sp. RCK2010
Fomitopsis cf. meliae 2IV 7 1
Fomitopsis sp. 9V 3 1 isolate 9V 3 1
Fomitopsis ostreiformis isolate BCC23382
Fomitopsis palustris...
0.01
Figure 1
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24
Figure 2
-
25
0
10
20
30
40
50
60
70
80
25 30 35 37 40 45
Temperature (C)
C
MC
ase
IU
/g
beta
-gl
uco
sida
se IU
/g
0
0.5
1
1.5
2
2.5
3
3.5
FP
ase
IU
/g
CMCase
Beta-glucosidase
FPase
Figure 3
-
26
Figure 4
-
27
Figure 5
-
28
0
50
100
150
200
250
0 4 8 12 16 20 24
Time (h)
Suga
r re
leas
ed (m
g/g)
Control RSNaOH treated RSAcid treated RSControl WSNaOH treated
WSAcid treated WS
Figure 6
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29
Table 1: Comparisons of cellulase production by Fomitopsis sp.
RCK2010 with other fungi under SSF
Enzyme Strain Activity (IU/g) Carbon Source Reference CMCase
Humicola lanuginosa 1.7 Beet pulp Grajek, W., 1986 Myceliophthora
sp. 26.6 Whaet bran Badhan et al., 2007
Pleurotus ostreatus IE8
Fomitopsis sp.RCK2010 0.18
71.699 Sugarcane bagasse
Wheat bran
Membrillo et al., 2008
Present work
FPase Myceliophthora sp. 0.74 Wheat bran Badhan et al., 2007
Pleurotus ostreatus IE8 0.013 Sugarcane bagasse Membrillo et al.,
2008 Thermoascus auranticus 4.4 Wheat straw Kalogeris et al., 2003
Fomitopsis sp.RCK2010 3.492 Wheat bran Present work -glucosidase
Humicola lanuginosa 46.8 Beet pulp Grajek, W., 1986 Sporotrichum
thermophile 12.1 Beet pulp Grajek, W., 1986 Myceliophthora sp. 3.83
Wheat bran Badhan et al., 2007 Fomitopsis sp.RCK2010 53.679 Wheat
bran Present work
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30
Table 2: Effect of substrate to moisture ratio on cellulase
production by Fomitopsis sp. RCK2010 under SSF
Enzyme Activity (IU/g) Substrate:Moisture CMCase FPase
-glucosidase
1:1 3.2850.094 0.1880.007 6.4310.154 1:1.5 4.0490.092 0.3190.024
26.0551.051 1:2 31.5441.415 1.2410.050 44.6750.953
1:2.5 71.0291.216 3.3080.010 51.8630.644 1:3 71.8760.460
3.2370.088 58.7770.776
1:3.5 72.5710.810 3.1910.035 66.5940.078 1:4 70.6690.942
2.4980.005 66.6080.151
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31
Table 3: Effect of different carbon sources on cellulase
production by Fomitopsis sp. RCK2010 under SSF
Enzyme Activity (IU/g) Carbon source (5g) CMCase FPase
-glucosidase
Corn cob 2.2150.040 0.1910.009 2.6580.067 Corn stover 3.6980.048
0.2430.032 2.7730.154 Wheat straw 2.4100.099 0.2390.013 3.2290.560
Prosopis juliflora 1.0520.071 0.7320.037 1.3930.098 Lantana camera
2.8950.097 0.4470.030 3.2270.086 Wheat bran 71.5260.910 3.2680.067
50.6960.662
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32
Table 4: Effect of different nitrogen source on cellulase
production by Fomitopsis sp. RCK2010 under SSF
Enzyme Activity (IU/g) Nitrogen source (0.05% N2 equivalent)
CMCase FPase -glucosidase
Control 71.6990.665 3.3190.004 51.4210.273 Inorganic
NaNO2 52.7781.095 4.4640.025 37.4120.800 NaN3 13.1660.398 0.000
0 KNO3 53.2650.596 3.4510.019 41.5490.725 Fe(NO3)3 46.3530.781
3.3590.024 41.9030.426 NH4Cl 46.8441.068 3.1500.023 47.6840.621
Ca(NO3)2 41.1250.955 3.1310.037 43.7791.094 (NH4)2C2O4 66.9740.489
4.5280.034 46.0760.954 NaNO3 57.8640.588 3.1730.018 47.5220.713
Pb(NO3)2 60.7990.325 2.6290.038 57.1140.889
Organic
Peptone 71.6500.636 4.3810.050 63.6930.668 Yeast extract
74.1631.015 4.3630.058 56.9770.409 Trytone 77.2580.873 4.1450.021
64.1260.936 Casein 71.5440.676 4.6820.037 64.9461.015 Soya been
meal 74.9960.520 4.1550.021 69.0830.904 Urea 81.8320.812 4.5620.029
54.9281.029 Corn steep liquor 70.8090.848 4.6430.032
52.1490.406
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33
Table 5: Effect of amino acids, vitamins and surfactants on
cellulase production by
Fomitopsis sp. RCK2010 under SSF
Enzyme Activity (IU/g) Additives (0.2%,)w/w CMCase FPase
-glucosidase
Control 71.6990.665 3.2690.067 51.9210.434
Aminoacids
L-Alanine 63.1600.443 5.0310.037 60.5240.713 L-Arginine
73.7561.063 4.9410.028 57.1160.893 L-Asparagine 77.8441.068
4.8340.011 65.9810.528 L-Aspartic Acid 79.0990.901 5.8340.011
61.0970.517 L-Cysteine 74.1670.397 5.1590.024 63.8890.839 L-Cystine
76.7991.042 6.1770.016 66.2110.100 L-Glutamic acid 84.1270.965
5.1090.071 61.7560.356 L-Glutamine 74.2480.826 4.8540.021
63.1040.991 Glycine 62.8250.561 6.2640.025 64.5430.680 L-Isoleucine
58.2910.853 5.0180.004 77.5460.733 L-Leucine 51.8480.543 3.4880.006
54.8150.384 L-lysine hydrochloride 56.3680.774 5.2730.013
65.2720.552 L-Methionine 35.0170.468 3.7480.018 51.9430.392
L-serine 64.1670.397 5.4470.030 66.2660.822 L-Threonine 72.0530.922
5.4470.022 62.0260.908 L-valine 61.7701.051 5.0460.022 61.6810.674
L-Phenylalanine 38.1150.893 4.0870.006 60.9680.928
4-hydroxy-L-proline 56.6940.670 6.7620.056 69.9950.898
L-Tryptophan 61.9581.015 3.6720.013 62.1050.422 L-Tyrosine
63.1330.940 4.0670.027 60.2630.590 L-Histidine hydrochloride
61.1230.477 5.9540.021 61.9970.941
Vitamins
Ascorbic acid 64.7791.099 5.6680.124 92.2512.244
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34
Riboflavin 65.7160.610 5.3770.107 73.0220.508 Retinol
51.0500.919 4.3650.172 73.4861.190 Biotin 52.5610.725 5.2250.158
86.6611.155 Folic acid 68.9780.529 2.6130.100 41.6641.153
Pyridoxine 33.7991.042 1.3660.177 20.6560.926 Thiamine 39.2470.878
1.5610.081 21.1260.607 Cyanocobalamine 35.9960.525 1.7840.088
22.2280.887
Surfactant
Tween-20 67.9231.498 4.7960.134 55.1951.322 Tween-40 74.9011.461
5.5510.324 56.3911.277 Tween-60 87.7911.560 5.5510.165 58.5681.618
Tween-80 89.5671.619 6.1180.149 61.7911.565 TritonX-100 98.2681.764
6.7110.156 65.3611.244 PEG-400 67.4551.200 3.5650.172 55.6621.725
PEG-4000 71.7191.551 4.2730.086 56.3601.245 PEG-6000 79.5441.210
5.1370.175 61.5021.650 PEG-8000 74.8651.478 4.6010.141
61.3651.242
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35
Table 6: Comparison of enzymatic hydrolysis of different
pretreated substrates by
cellulases from different fungi and commercial preparations
Source Substrate Reducing sugar (mg/g of substrate)
Reference
L. sulphureus Pinus densiflora 70.9 Lee et al., 2008 Trichoderma
reesei and Novozyme 188 Trichoderma reesei and Novozyme 188
Trichoderma reesei and Novozyme 188
Corn cob Prosopis
Lantana
826.2 838.9 777.6
Gupta et al., 2011
Gupta et al., 2011 Gupta et al., 2011
Fomitopsis pinicola Pinus densiflora 3.5 Lee et al., 2008
Fomitopsis palustris
Fomitopsis sp.RCK2010 Fomitopsis sp. RCK2010
Avicel
Rice straw Wheat straw
32
157.2 214.1
Yoon et al., 2005 Present work
Present work