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CIVIL, ENVIRONMENTAL &
GEOMATIC ENGINEERING
DEPARTMENT
EVALUATION OF FINE SAND FILTRATION FOR
LARGE SCALE ALGINATE PURIFICATION FOR
CLINICAL USE
M.SC. DISSERTATION
TIMEA GREGO
M.SC. ENVIRONMENTAL SYSTEMS ENGINEERING
SUPERVISED BY: DR LUIZA CINTRA CAMPOS
DR CLARE SELDEN
London, 31st August 2009
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EVALUATION OF FINE SAND FILTRATION FOR LARGE SCALE ALGINATE PURIFICATION FOR CLINICAL USE
TIMEA GREGO II
MSc DISSERTATION SUBMISSION
Student Name: TIMEA GREGO
Programme: M.Sc. Environmental Systems Engineering
Supervisors: Dr Luiza C Campos
Dr Clare Selden
Dissertation Title:
EVALUATION OF FINE SAND FILTARTION FOR LARGE SCALE ALGINATE
PURIFICATION FOR CLINICAL USE
DECLARATION OF OWNERSHIP
I confirm that I have read and understood the guidelines on plagiarism, that I understand the
meaning of plagiarism and that I may be penalised for submitting work that has been
plagiarised.
I declare that all material presented in the accompanying work is entirely my own work except
where explicitly and individually indicated and that all sources used in its preparation and all
quotations are clearly cited.
Should this statement prove to be untrue, I recognise the right of the Board of Examiners to
recommend what action should be taken in line with UCL‟s regulations.
Signature: Date:
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EVALUATION OF FINE SAND FILTRATION FOR LARGE SCALE ALGINATE PURIFICATION FOR CLINICAL USE
TIMEA GREGO III
This M.Sc. Thesis was a collaboration between the Centre for Hepatology at the Royal Free
University College London (UCL) - Royal Free Hospital Campus, and the Civil,
Environmental and Geomatic Engineering Department, UCL.
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TIMEA GREGO IV
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TIMEA GREGO V
THIS THESIS IS DEDICATED TO THE LOVING MEMORY OF MY FATHER,
JÁNOS GREGÓ (1955-1989)
DIPLOMAMUNKÁMAT ÉDESAPÁM EMLÉKÉNEK AJÁNLOM
GREGÓ JÁNOS (1955-1989)
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ABSTRACT
Alginate is a natural polysaccharide, harvested from brown seaweed. Tissue engineering and
medical science mainly utilise its gel-forming “ability in the presence of various divalent
cations” [1]. In this project, alginate is used to microencapsulate HepG2 cells for use in a
Bioartificial Liver machine. Therefore, biocompatibility of alginates for immobilising
hepatocytes is crucial. Several in house purification methods were published, which tried to
achieve a suitable biocompatibility of the polymer by removing the known impurities i.e.
proteins and endotoxins, but failed to maintain the physical properties of alginate solution.
In this study, an attempt was made to purify research grade sodium alginate solution from
“unknown” (micron particulate) impurities by fine sand filtration [2]. For clinical application
through regulatory, authority approval particulates must be removed to prevent transit to the
patient.
The hypothesis was that the sand filtration will remove particulates between 1µm to 10µm
from the solution without inducing physical changes in the polymer solution. The specific
aims were
1. To evaluate the effect of fine sand filtration on the sodium alginate solution‟s
properties.
2. To determine, measure any changes in the physical properties of the non-Newtonian
fluid by rheology.
3. Encapsulate empty alginate beads to assess morphology of beads after filtration.
4. To immobilise encapsulated HepG2 cells in filtered alginate solution and compare
with non filtered alginate encapsulated HepG2 cells using cell growth, viability and
function as comparators.
The results showed that micron particulates removal efficiency of dual media filtration was
higher compared to mono medium filter. However, the purification method of the polymer
had negatively influenced the dynamic viscosity of the solution, thereby altering the
functional properties of the hydrogels.
As can be seen, the hypothesis was not proven in the large scale purification of alginate for
clinical use. The research outcomes highlighted the need for an alternative approach to purify
alginate solution, which could be achieved by utilising the gas-solid separation method of dry
alginate powder.
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TIMEA GREGO VII
ACKNOWLEDGEMENTS
My sincerely appreciation goes to my supervisors, Dr Luiza Campos and Dr Clare Selden, for
their support and encouragement during my research work. I highly appreciate both of you for
giving me the opportunity to work on a multidisciplinary research project. Thank you very
much.
I would also like to thank to Amir Gander, for his continuous support, patient and guidance.
Dear Amir, I really appreciate all the help you gave me. You have never let me down and I
thank you very much for this.
I extend my appreciation to the people at the Environmental Engineering Laboratory and
Department of Pharmacology at University College London (UCL), and Hepatology
Laboratory at Royal Free Hospital for their support. I also want to thank to Dr Arnold
Darbyshire for giving the opportunity to use the rotational viscometer at University College
Medical School at the Department of Surgery, Royal Free Hospital.
I would like to express my appreciation to Matt Kite and Graeme Oakes at PAMAS
Partikelmess- und Analysesysteme GmbH for providing the Liquid particle counting
apparatus. I would also like to thank to Sibelco UK Ltd. for supplying the sand samples for
the experiment.
Special acknowledgement goes to, Mr Ian Sturtevant, at University College London, Civil,
Environmental Engineering and Geomatic Engineering Department for his support, time and
technical advice.
I would like to record my appreciation to University of Miskolc, Hungary for providing me
with a solid engineering and science knowledge.
I would like to thank to all my friends for encouraging and helping me during the M.Sc.
course.
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TIMEA GREGO VIII
Dear Mummy, I would like to thank you for bringing me up with the greatest love and care. I
really appreciate your support and care. I am so proud of you! Without you, I would not be
the person who I am. Also, I extend my gratitude to my sisters, Erika and Marianna, for their
love and understanding.
As well, I must not forget my loved ones who cannot be with me. Dear Daddy, I have
inherited the strength and passion for science and engineering from you. Your love and
support was always by my side. I miss you so much!
Drága Édesanya, szeretném megköszönni, hogy a legnagyobb szeretetben és gondoskodásban
neveltél fel. Büszke vagyok rád! Merhetettlenül hálás vagyok, a mindenkori támogatásodért
és megértésedért. Nélküled nem lehetnék az, aki vagyok.
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CONTENTS
ABSTRACT ............................................................................................................................................. VI
LIST OF FIGURES .................................................................................................................................. XII
LIST OF TABLES ................................................................................................................................. XVI
NOMENCLATURE ............................................................................................................................... XVII
LIST OF ABBREVATIONS................................................................................................................... XVIII
1 INTRODUCTION .............................................................................................................................. 1
2 RESEARCH GOALS AND APROACH ................................................................................................ 5
2.1 AIMS OF THE INVESTIGATION AND APPROACH ......................................................................... 5
3 LITERATURE REVIEW ................................................................................................................... 6
3.1 ALGINATE - NATURAL POLYMER ............................................................................................. 6
3.2 STRUCTURE AND PROPERTIES OF ALGINATE ........................................................................... 8
3.3 CHARACTERISTIC AND PROPERTIES OF ALGINATE ................................................................... 9
3.3.1 MOLECULAR WEIGHT ...................................................................................................... 9
3.3.2 SOLUBILITY ................................................................................................................... 10
3.3.3 GEL FORMATION ............................................................................................................ 10
3.3.4 VISCOSITY ..................................................................................................................... 11
3.4 PURIFICATION METHODS OF ALGINATE FOR CLINICAL USE ................................................. 13
3.5 FINE SLOW SAND FILTRATION PROCESS ................................................................................ 11
3.5.1 PHYSICAL PARAMETERS AFFECT THE OPERATION OF FILTER MEDIA ............................ 12
3.5.2 MECHANISM OF FILTRATION ......................................................................................... 13
3.5.3 TYPES OF GRANULAR MEDIA FILTERS ........................................................................... 21
3.5.4 HYDRAULICS OF SAND FILTER ....................................................................................... 24
3.5.5 TIME-INDEPENDENT NON-NEWTONIAN FLUIDS ............................................................ 26
4 MATERIAL AND METHODS ......................................................................................................... 30
4.1 PREPARATION OF 2% HEPES BUFFERED ALGINATE SOLUTION ............................................. 31
4.2 TESTING OF FILTER MEDIA ..................................................................................................... 32
4.2.1 CHEMICAL ANALYSIS OF FILTER MEDIA ........................................................................ 32
4.2.2 PHYSICAL ANALYSIS OF FILTER MEDIA ......................................................................... 32
4.2.3 SETTLING VELOCITY OF INDIVIDUAL GRAINS................................................................ 33
4.2.4 SHAPE (SPHERICITY) OF FILTER MEDIA ......................................................................... 33
4.2.5 POROSITY OF FILTER MEDIA .......................................................................................... 34
4.2.6 DETERMINATION OF HEADLOSS IN CLEAN GRANULAR MEDIA FILTER .......................... 34
4.3 SYSTEMS PREPARATION FOR FILTRATION .............................................................................. 35
4.3.1 TREATMENT OF FILTER MEDIA BEFORE USE .................................................................. 35
4.3.2 TREATMENT OF THE FILTRATION SYSTEMS BEFORE USE ............................................... 35
4.4 FILTRATION SYSTEMS INSTALLATION .................................................................................... 35
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4.5 SAND FILTRATION EXPERIMENT ............................................................................................. 40
4.5.1 FILTERED AQUEOUS SODIUM-ALGINATE SAMPLES ........................................................ 41
4.5.2 SODIUM ALGINATE VISCOSITY MEASUREMENT ............................................................. 43
4.5.3 TURBIDITY ..................................................................................................................... 43
4.6 LYOPHILISATION OF FILTERED SODIUM-ALGINATE ................................................................ 43
4.7 RECONSTRUCTION OF SODIUM-ALGINATE ............................................................................. 45
4.7.1 ANALYTICAL CENTRIFUGATION .................................................................................... 45
4.7.2 DETERMINATION OF THE SIZE DISTRIBUTION OF THE PARTICULATES ........................... 46
4.7.3 ENCAPSULATION OF FILTERED SODIUM-ALGINATE ....................................................... 46
4.8 ENCAPSULATION OF HEPG2 CELLS ........................................................................................ 47
5 EXPERIMENTAL RESULTS AND DISCUSSION............................................................................... 48
5.1 TESTING OF FILTER MEDIA ..................................................................................................... 48
5.1.1 PHYSICAL ANALYSIS OF FILTER MEDIA ......................................................................... 48
5.1.2 SPHERICITY (SHAPE) OF FILTER MEDIA ......................................................................... 51
5.1.3 SETTLING VELOCITY OF INDIVIDUAL GRAINS................................................................ 51
5.1.4 POROSITY OF FILTER MEDIA .......................................................................................... 52
5.2 HYDRAULIC OF FILTRATION ................................................................................................... 55
5.2.1 DETERMINATION FLOW REGIMES AND DRAG COEFFICIENT .......................................... 55
5.2.2 DETERMINATION OF CLEAN-WATER HEAD LOSS IN GRANULAR-MEDIA FILTER .......... 57
5.2.3 TURBIDITY ..................................................................................................................... 61
5.3 EVALUATION OF THE VISCOSITY MEASUREMENTS OF SODIUM ALGINATE SOLUTIONS .......... 62
5.3.1 EFFECT OF DIFFERENT CONCENTRATION ON SOLUTION VISCOSITY .............................. 63
5.3.2 EFFECT OF AUTOCLAVING ON SOLUTION VISCOSITY..................................................... 65
5.3.3 EFFECT OF TEMPERATURE ON SOLUTION VISCOSITY..................................................... 66
5.3.4 EFFECT OF FILTRATION ON THE SOLUTION VISCOSITY .................................................. 67
5.4 RECONSTRUCTION OF SODIUM-ALGINATE ............................................................................. 69
5.4.1 EVALUATION OF THE EFFECT OF FINE SAND FILTRATION ON THE SIZE DISTRIBUTION OF
THE PARTICULATES ....................................................................................................................... 69
5.4.2 EVALUATION OF PARTICLE SIZE MEASUREMENT OF FILTERED SODIUM ALGINATE
SOLUTIONS .................................................................................................................................... 73
5.4.3 ENCAPSULATION OF FILTERED SODIUM-ALGINATE ....................................................... 74
5.5 ENCAPSULATION OF HEPG2 CELLS ........................................................................................ 76
5.5.1 MORPHOLOGY OF CELL CULTURED ALGINATE BEADS .................................................. 76
5.5.2 PROTEIN PRODUCTION FROM ENCAPSULATED HEPG2 CELL ......................................... 77
5.5.3 ASSESSMENT OF CELL VIABILITY IN ALGINATE BEADS ................................................. 78
6 CONCLUSIONS .............................................................................................................................. 81
7 RECOMMENDATIONS ................................................................................................................... 84
7.1 OPERATION OF THE GAS-SOLID CYCLONE .............................................................................. 85
REFERENCES ........................................................................................................................................ 88
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LIST OF FIGURES
PHOTOGRAPHS: All of the photographs for this dissertation were taken by Timea Grego, unless
otherwise stated.
FIGURE 1.1 THE THREE PHASES OF THE BAL SYSTEM
FIGURE 3.1 LAMINARIA GENERA
FIGURE 3.2 MONOMER SALTS OF ALGINATE
FIGURE 3.3 SHEAR RATE VERSUS VISCOSITY OF DIFFERENT ALGINATE
SOLUTION CONCENTRATION
FIGURE 3.4 CORRELATION BETWEEN TEMPERATURE AND THREE
DIFFERENT 1% ALGINATE SOLUTION
FIGURE 3.5 SOLUTION CONCENTRATION EFFECTS ON THE POLYMER
VISCOSITY
FIGURE 3.6 HYDRAULICS OF A FLUID THROUGH PERMEABLE MEDIA
FIGURE 3.7 DRAG COEFFICIENT (CD) FOR SPHERES AS A FUNCTION OF
RE OVER LAMINAR-, TRANSITION- AND TURBULENT
FLOW REGIMES. IT CAN BE SEEN FROM THE FIGURE, THAT
RE INCREASES WITH DECREASING CD.
FIGURE 3.8 GRAVITATION FORCE (FG), BUOYANT FORCE (FB) AND
DRAG FORCE (FD) AFFECT THE MOTION OF A PARTICLE IN
WATER DURING SEDIMENTATION
FIGURE 3.9 TRANSPORT MECHANISMS DURING FILTRATION
FIGURE 3.10 ELECTRICAL DOUBLE LAYER
A) ELECTROSTATIC FIELD AROUND AN ANIONIC PARTICLE
B) ILLUSTRATION OF ZETA POTENTIAL, SHEAR
PLANE, AND ELECTROSTATIC POTENTIAL
FIGURE 3.11 DIFFERENT SEPARATION PROCESSES IN ACCORDANCE
WITH THE SIZE DISTRIBUTION OF POSSIBLE IMPURITIES
PRESENT IN WATER
FIGURE 3.12 DIFFERENT SAND FILTER MEDIA SYSTEMS
FIGURE 3.13 VISCOSITY OF NEWTONIAN FLUIDS
FIGURE 3.14 FLOW CURVE OF NEWTONIAN FLUIDS
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FIGURE 3.15 FLOW CURVES OF VARIOUS TIME-INDEPENDENT NON
NEWTONIAN FLUIDS
FIGURE 4.1 LIFE CYCLE OF THE EXPERIMENTAL WORK
FIGURE 4.2 PHASE I. FILTRATION: SMALL SCALE SYSTEM BEFORE
THE FILTER MEDIA INSTALLATION
FIGURE 4.3 PHASE IV. FILTRATION: LARGE SCALE, SINGLE MEDIA
FILTRATION SYSTEM
FIGURE 4.4 PHASE IV. FILTRATION: DUAL MEDIA FILTRATION
SYSTEM
FIGURE 4.5 SHELL FREEZING PROCESS OF FILTERED NA-ALGINATE
SOLUTION
FIGURE 4.6 DRIED ALGINIC ACID AFTER LYOPLISIATION
FIGURE 4.7 ANALYTICAL CENTRIFUGE ANALYSIS BY EPPENDORF
CENTRIFUGE 5415R
FIGURE. 5.1 GRAIN SIZE DISTRIBUTION GRAPH OF RH-70
PARTICLE SIZES (µM) VERSUS CUMULATIVE PASSING OF
THE GRAINS (%)
FIGURE. 5.2 GRAIN SIZE DISTRIBUTION GRAPH OF RH-110 PARTICLE
SIZE (µM) VERSUS CUMULATIVE PASSING OF THE
PARTICLES
FIGURE 5.3 MASS –VOLUME RELATIONSHIP OF A SEDIMENT SAMPLE
FIGURE 5.4 (A-F) VOLUMETRIC FLOW RATES VERSUS SAMPLING
DATES DURING PHASE I-III AND V. FILTRATION PERIODS
FIGURE 5.5 A-D FLOW CURVES OF NEWTONIAN AND TIME-
INDEPENDENT NON-NEWTONIAN FLUIDS
FIGURE 5.6 DYNAMIC VISCOSITY OF 0.2% NAALG SOLUTION AS A
FUNCTION OF SHEAR STRESS (PA)
FIGURE 5.7 FLOW CURVES OF AUTOCLAVED NAALG (CONTROL)
SOLUTIONS
FIGURE 5.5 A-D FLOW CURVES OF NEWTONIAN AND TIME-
INDEPENDENT NON-NEWTONIAN FLUIDS
FIGURE 5.6 DYNAMIC VISCOSITY OF 0.2% NAALG SOLUTION AS A
FUNCTION OF SHEAR STRESS (PA)
FIGURE 5.7 FLOW CURVES OF AUTOCLAVED NAALG (CONTROL)
SOLUTIONS
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TIMEA GREGO XIV
FIGURE 5.8 VISCOSITY OF 2% NAALG SOLUTION AT DIFFERENT
TEMPERATURES
FIGURE 5.9 FLOW CURVES OF 2% NAALG SOLUTION AT DIFFERENT
TEMPERATURES
FIGURE 5.10 FLOW CURVES OF FINE SAND FILTERED 0.2% NA-
ALGINATE SOLUTIONS
FIGURE 5.11 FLOW CURVES OF MONO MEDIUM AND DUAL MEDIA
FILTERED 0.2% NA-ALGINATE SOLUTIONS
FIGURE 5.12 PARTICLE SIZE DISTRIBUTION OF NON-PURIFIED 2%
SODIUM ALGINATE SOLUTION
FIGURE 5.13 LENGTH DISTRIBUTION (µM) OF PARTICLES IN RH-70
SAND FILTERED NAALG SOLUTION. (A) PARTICLES
LENGTH UNDER SLOW FLOW RATE (B) PARTICLES
LENGTH UNDER INCREASED FLOW RATE
FIGURE 5.14 LENGTH DISTRIBUTION (µM) OF PARTICLES IN RH-110
SAND FILTERED NAALG SOLUTION. (A) PARTICLES
LENGTH UNDER SLOW FLOW RATE (B) PARTICLES
LENGTH UNDER INCREASED FLOW RATE
FIGURE 5.15 PARTICLES LENGTH DISTRIBUTION (µM) OF LARGE SCALE
FINE SAND FILTERED NAALG SOLUTION
FIGURE 5.16 DISTRIBUTION OF PARTICLES SIZES (µM) AND NUMBERS
OF NA-ALGINATE POWDER
FIGURE 5.17 ALGINATE BEADS FROM NON-PURIFIED 2% SODIUM
ALGINATE SOLUTION
FIGURE 5.18. EFFECT OF THE NA-ALGINATE SOLUTION
CONCENTRATION ON THE MORPHOLOGY AND SIZE OF
EMPTY ALGINATE BEADS. BEADS WERE PREPARED USING
1.25% (A) AND 1.5% (B) DMF FILTERED SOLUTION; C
1.75% MMF FILTERED SOLUTION AND D 2% FINE SAND
FILTERED AQUEOUS NA-ALGINATE.
FIGURE 5.19 PHASE 4: ENCAPSULATED HEPG2 CELLS; MONO MEDIUM
FILTERED 1.875% SODIUM ALGINATE SOLUTION WAS
USED FOR CELL IMMOBILISATION
FIGURE 5.20 PHASE 4: ENCAPSULATED HEPG2 CELLS; DUAL MEDIA
FILTERED 1.875% SODIUM ALGINATE SOLUTION WAS
USED FOR CELL IMMOBILISATION
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FIGURE 5.21 ALBUMIN (PROTEIN) PRODUCTION FROM ENCAPSULATED
HEPG2 CELLS IN A NON FILTERED, MONO MEDIUM, AND
DUAL MEDIA FILTERED ALGINATE SOLUTION
FIGURE 5.22 VIABILITY OF ENCAPSULATED HEPG2 CELLS IN A NON
FILTERED AND MONO MEDIUM, AND DUAL MEDIA
FILTERED ALGINATE SOLUTION
FIGURE 5.23 CELLS NUMBER OF PURIFIED AND NON PURIFIED
ALGINATE ENCAPSULATED HEPG2 CELLS
FIGURE 5.24 LIVE AND DEAD ENCAPSULATED HEPG2 CELLS IN MONO
MEDIUM AND DUAL MEDIA FILTERED ALGINATE
MICROCAPSULES AT DAY 3 STAINED WITH FDA AND PI.
FIGURE 7.1 PARTICLE SIZE DISTRIBUTION OF SEVERAL MATERIALS IN
A FUNCTION OF SEPARATION TECHNIQUE; CYCLONES
SEPARATION PARTICLE SIZE 1µM-1,000µM [66].
FIGURE 7.2 REVERSE FLOW CYCLONE SEPARATOR. SUSPENDED
PARTICLES IN GAS ENTER IN THE CYCLONE AND
CENTRIFUGAL FORCES (VORTEX) DRIVE THEM TO THE
CENTRAL PART, WHERE THE PARTICLES WILL BE
SEPARATED.
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LIST OF TABLES
TABLE 1.1 SPECIFICATION OF SODIUM-ALGINATE
TABLE 3.1 APPLICATION OF ALGINATE BY ITS CHARACTERISTICS
AND FUNCTIONALITY
TABLE 3.2 M, G AND MG FRACTION COMPOSITION OF
COMMERCIALLY AVAILABLE ALGAL ALGINATES
TABLE 3.3 SPHERICITY OF SAND
TABLE 3.4 POROSITY OF SAND
TABLE 3.5 DESIGN PARAMETERS OF SINGLE-MEDIUM, DUAL-, AND
MULTI-MEDIA FILTERS
TABLE 4.1 WATER QUALITY PARAMETERS OF MILLI-Q WATER
TABLE 4.2 FILTERED NA-ALGINATE SAMPLES DURING THE FINE
SAND FILTRATION PERIODS
TABLE 5.1 REDUCED DATA OF GRAIN SIZE DISTRIBUTION ANALYSIS
OF RH-70 (COARSE SAND) AND RH-110 (FINE SAND)
TABLE 5.2 DETERMINED DENSITY OF RH-70 FILTER MEDIUM
COMPARED TO DATA AVAILABLE IN LITERATURE
TABLE 5.3 ESTIMATED SPHERICITY OF RH-70 AND RH-110
COMPARED TO DATA AVAILABLE IN LITERATURE
TABLE 5.4 AVERAGE SETTLING VELOCITY OF COARSE AND FINE
SAND GRAINS
TABLE 5.5 ESTIMATED POROSITY OF RH-70 AND RH-110
TABLE 5.6 PHYSICAL PARAMETERS OF THE FILTER MEDIA
TABLE 5.7 ESTIMATED SPHERICITY VALUE AND CALCULATED
EQUIVALENT HYDRAULIC DIAMETER
TABLE 5.8 VOLUMETRIC FLOW RATES, APPROACH VELOCITIES AND
HEADLOSSES DURING FILTRATION
TABLE 5.9 TURBIDITY LEVEL AND CONCENTRATION (NTU) OF THE
EFFLUENT SAMPLES AFTER BACKWASHING
TABLE 5.10 PREPARED SAMPLES FOR VISCOSITY ANALYSIS
TABLE 5.11 EFFECT OF AUTOCLAVING AT 121°C FOR 10 AND 20MINS
ON THE VISCOSITY OF NAALG SOLUTIONS
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NOMENCLATURE
DEFINITION SYMBOL UNIT
GRAVITY g
s
m81.9
SETTLING VELOCITY tv
s
m
APPROACH VELOCITY OF FILTRATION v
s
m
HYDRAULIC DIAMETER d m
FILTER DIAMETER fd m
SIEVE SIZE Sd m
REYNOLDS‟ NUMBER R DIMENSIONLESS
DRAG COEFFICIENT DC DIMENSIONLESS
HEAD LOSS OF THE SAND h m
HEIGHT OF THE SETTLING COLUMN SCh m
BED DEPTH L m
AVERAGE TIME tav [s]
POROSITY OF THE GRANULAR MEDIA n [%]
GREEK SYMBOLS
DENSITY OF WATER AT 20°C1 )20(2 CTOH
998.23
3m
kg
ABSOLUTE VISCOSITY OF WATER AT
20 °C )20(2 CTOH
sPa
sm
kg3100087.1
ABSOLUTE VISCOSITY OF SODIUM
ALGINATE (NaAlg) lgNaA
sPa
sm
kg
GRAIN SPHERICITY OR SHAPE FACTOR Ψ DIMENSIONLESS
DENSITY OF SAND S
32650
m
kgS
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LIST OF ABBREVATIONS
AMC-BAL Amsterdam Medical Centre-bioartificial liver
ASTM American Standards for Testing
BAL BioArtificial Liver
DMF Dual Media Filter (RH-70&RH-110)
ELAD
EMEA European Medicines Agency
FDA Food and Drugs Administration
FDA Fluorescein diacetate
GRAS Generally Recognised as Safe
MELS Modular extracorporeal liver system
MHRA Medicines and Healthcare products Regulatory Agency
MMF Mono Medium Filter (RH-110)
NaAlg Sodium alginate
PI Propidium iodide
TEMPS Tissue-Engineered Medical Products
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1 INTRODUCTION
This dissertation focuses on the large scale purification treatment of research-grade sodium
alginate (NaAlg) for clinical use. Alginate is a natural biopolymer extracted from brown
seaweed, and used for encapsulation of living cells, thereby allowing their use within a
bioartificial (BAL) device.
Liver disease is the only major cause of death which increases every year in the UK. The
Office of National Statistics reported in September 2008 that liver disease caused an
estimated 161 deaths/million population of male and 78 deaths/million population of
female deaths [3]. Acute Liver failure is often classified as severe liver disease symptoms
(jaundice, encephalopathy) with an 80-90% reduction in liver cell numbers, which has
many causes including alcohol abuse, infection, genetic causes, with a mortality rate of
between 70-90%. Chronic liver disease is often attributed to cirrhosis of the liver,
developed over time often due to alcohol abuse, non-alcoholic steatohepatitis, and chronic
hepatitis [4]. For patients today the only possible treatments are an organ transplantation,
or spontaneous liver regeneration.
Scientists and researchers are continuously seeking to develop non-biological or biological
liver support systems to treat patient with hepatic failure. Non-biological systems classified
as “plasma exchange, albumin dialysis, hemo(dia)filtration, and adsorbent based devices”
[5] provide only blood detoxification. Functions of liver are so complex when hepatic
failure occurs; the accumulated endotoxin, cell growth inhibitors and various known and
unknown materials cause “neurological abnormalities to the liver” and other internal
organs [5]. It is difficult to purify the blood from these compounds by using conventional
treatment methods. Therefore, to fulfil the complex function more advanced hepatocyte
based devices have been developed, such as
ELAD, which is a hollow-fibre bioreactor and contains human C3A cell line,
Modular extracorporeal liver system (MELS) a complex system in which “four
interwoven hollow-fibre capillary systems carry out independent functions”;
Amsterdam Medical Centre-bioartificial liver (AMC-BAL) loaded with “10-14
billion immobilised porcine hepatocytes on a spirally wound polyester fabric”;
HepatAssistTM
device was the first BAL system in “FDA-approved clinical trials”
[5].
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The Liver Group has developed a Bioartificial Liver Device (BAL) that aims to bridge the
gap between diagnosis and transplantation or aid spontaneous regeneration. This BAL
system consists of three phases (Figure 1.1) Phase 1 HepG2 (a human hepatocyte immortal
cell line) cells are encapsulated in alginate beads achieving a 3D state, which provides
better cell growth and function [6]. For immobilisation of HepG2 cells purified alginate is
required; Phase 2 Encapsulated cells are proliferated in a Fluidised Bed Bioreactor over 8-
10 days; Phase 3 patient plasma is passed over beads by fluidisation [7].
Figure 1.1 THE THREE PHASES OF THE BAL SYSTEM
PHASE 1 HEPG2 CELLS ARE ENCAPSULATED IN ALGINATE BEADS; PHASE 2 ENCAPSULATED CELLS
ARE PROLIFERATED IN A FLUIDISED BED BIOREACTOR OVER 8-10 DAYS; PHASE 3 PATIENT PLASMA
IS PASSED OVER BEADS BY FLUIDISATION.
“(i.) FDA STAINED HEPG2 CELLS AFTER ENCAPSULATION. (ii.) FDA STAINED HEPG2 CELLS AFTER
8 DAYS OF PROLIFERATION. (iii.) A PHASE CONTRAST ALGINATE BEADS 8 DAYS AFTER INITIAL
IMMOBILISATION. (iv.) FLUIDISED BED BIOREACTOR (FBB) COMPETENCE CULTURE SETUP. (v.)
FBB CONTAINING ALGINATE” [8].
Phase I. Phase II. Phase III.
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The biomedical application of alginate for regulatory approval requires the production of a
highly purified polysaccharide. Sodium alginate (Table 1.1) is listed as “direct food
materials affirmed as Generally Recognised as Safe (GRAS)” by the American Food and
Drug Administration (FDA) [9]. In addition to the Food and Drug Administration, USA
(FDA), the European Medicines Agency (EMEA) and the Medicines and Healthcare
products Regulatory Agency (MHRA), and The American Society for Testing and
Materials (ASTM) have also established standards and guidelines for biopolymers in
Tissue-Engineered Medical Products (TEMPs). „ASTM Alginate and Chitosan Standard
Guide‟ provides information on the physical and chemical properties for the biomaterial
[10]. Moreover, Alginate is referenced in the European, British, and United States
Pharmacopoeia and The Complete Drug Reference Book [11-12].
TABLE 1.1 SPECIFICATION OF SODIUM ALGINATE [13]
SODIUM – ALGINATE (NAALG)
CHEMICAL FORMULA n
NaOHC 676
STRUCTURE OF ALGINATE
PROPERTIES OF THE POLYMER Stabilizer, thickener and ability to form gels in the presence of
divalent cations
As an existing scaffold material for immobilising living liver cells, the purity level of the
biopolymer is crucial. According to recent research, alginate may contain “unknown” and
known “contaminants” [2]. The former can be classified as micron particulates, and the
latter as heavy metals, endotoxins, proteins, pyrogens, and polyphenols [14].
Numerous works have been published on the efficient reduction of “known” impurities
from alginates such as free flow electrophoresis (FFE) and multi-step chemical
purification, which utilises chemical treatments [15]. Alginate purified by FFE treatment is
not suitable for clinical use because the process is time consuming and prohibitively
expensive. An advantage of the multi-step chemical approach compared to FFE is that
alginate can be created with different mannuronic (M)- and guluronic (G) acid ratios [15].
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The most commonly detected impurities (endotoxin, proteins and polyphenols) can be
eliminated by these purification methods [2]. However, it is important to note that viscosity
of the polymer changes during the purification process for both FFE and multi-step
chemical treatment, which would impact on the functionality within the Liver Group BAL.
An alternative treatment method (Depth Charged Filtration) of 0.2% Na-alginate solution
was tested at UCL Medical School, Royal Free Campus. Zeta Plus Maximizer Dual-Zone
Depth Filters were used, which utilise a cellulose based filtration system. The filter media
is positively charged thus allowing the removal of anionic impurities such as cellular
debris, endotoxins and viruses from the solution [16]. Although it removed larger
particulates, viscosity of the filtered Na-alginate solution was changed as a result of the
filtration process, and made the purified biopolymer unsuitable for cell encapsulation. As
can be seen, during the depth filtration the same problem emerged compared to the
previously described purification processes.
It has become clear after an interdisciplinary literature review, that there is little
precedence for removal of micron particulates („unknown‟ contaminants) using sand
filtration, from analytical grade material for use in a clinical environment. Therefore, fine
sand filtration process was chosen because it does not require pre-treatment of the influent
and it is easy to operate compared to the published in-house alginate purification methods
[2, 17, 14, 18-20].
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2 RESEARCH GOALS AND APROACH
2.1 Aims of the investigation and approach
The aim of this dissertation was to explore the hypothesis that sand filtration will remove
particulates from alginate solutions without altering the viscosity of the resultant solution
The specific aims of the research project were:
To remove micro particulates from 1µm to less than 10µm.
To evaluate the effect of filter media size on the micro-particulates removal.
To determine the effect of flow rate and sand depth on particulates removal efficiency.
To measure the viscosity of the non-Newtonian fluid during the treatment process life-
cycle, to indicate changes in alginate composition.
To determine the particle size distribution of micron particulates, which validates the
efficiency of filtration.
To use the filtered alginate for the encapsulated HepG2 cells.
To evaluate the effects of different sodium-alginate concentrations on the bead shape,
if bead integrity is compromised.
To evaluate the growth and function of the encapsulated cells over 15 days.
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3 LITERATURE REVIEW
The present research is a multidisciplinary project incorporating medical science and
engineering. To understand the complexity of the research project, the holistic nature of the
project was investigated. There were three dimensions of this view
Spatial aspect, in which an investigation was undertaken to determine the link
between this research environment in a global context, by establishing the reason
for the study.
Temporal view, which requires investigating the research project in terms of the
past, present and future.
System dimension, which aimed to demonstrate the interaction between the sub –
system and the super system and helped to build up a critical picture of the problem
statement [21].
3.1 Alginate - Natural Polymer
Sodium Alginates (polysaccharide) are salts of alginic acid which is a natural polymer
abundant in nature. The polysaccharide is commonly extracted from marine brown algae of
class Phaeophyceae, providing a structural component of the plant and is also synthesised
by the soil bacteria and more environmentally common Pseudomonas aeruginosa cellular
polyose in soil bacteria [22-23]. Commercially available alginate is extracted from a
particular brown seaweed of genus of Macrocystis, and Laminaria (Figure 3.1).
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FIGURE 3.1. LAMINARIA GENERA [24]
In recent decades, the demand for alginate production has increased rapidly. The medical,
pharmaceutical, food and industries utilise the functional properties of alginate, such as
solubility in water, gelling, thickener and stabilising effects (Table 3.1). Most relevantly,
biomedical and pharmaceutical industries often use alginate as scaffolds in tissue
engineered medical products [10] and for cell implantation [25], using medical grade
alginate, which is a highly purified form.
TABLE 3.1 APPLICATIONS OF ALGINATES BY ITS CHARACTERISTICS AND FUNCTIONALITY [26]
CHARACTERISTICS FUNCTIONALITY BENEFITS APPLICATIONS
MOLECULAR WEIGHT Viscosity Thickening, film-
forming
Suspensions, coatings
COMPOSITION AND
SEQUENCE
Cross-linking Gelling Immobilization,
encapsulation
DISSOCIATION, PKA Soluble at pH,
precipitate at pH,
swelling capability
Solutions, fibers, films,
adsorption
Solutions, pastes,
scaffolds, dressings,
membranes, tablet
disintegration
POLYANION Cation affinity Chelation Gelation, drug, metal
binding
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3.2 Structure and Properties of Alginate
Alginates are non-branched binary copolymers consisting of two residues namely, β-D-
mannuronic acid (M) and α-L- guluronic acid (G), linked by a (1→4) glycoside bonds [10,
26, 27]. During the extraction of the carbonhydrate polymers, the mannuronic and
guluronic acids are converted into mannuronate (M) and guluronate (G) salts (Figure 3.2).
It has been reported that the structural differences of the two uronic acids monomers are
minor thus they form different chair conformations [27].
Physical properties of the hydrogel depend on the block structure and composition of
alginate. Determination of diad (FGG, FGM, FMG and FMM), triad (FGGG, FGGM, FMGG, FMGM,
FMMM, FMMG, FGMM, and FGMG) and higher order frequencies of the monomer composition
by NMR spectroscopy allows the calculation of average block length [28].
The G- content, the length of the G-block and molecular weight determine the gelling
properties of alginate. Table 3.2 shows the composition and block structure in different
sources of alginate. Na-alginate is used as an encapsulation medium for HepG2 cells,
which seeks to provide the cell component for the BAL. The main advantage of the
polymer is to provide supporting environment for the encapsulated cells therefore,
promoting growth and function of HepG2 cells compared with monolayer.
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FIGURE 3.2 MONOMER SALTS OF ALGINATE [29]
Alginate is a block copolymer, hence monomer rings are distributed within the polymer in
diverse sequence and can be described by three block structures. These are homo-
polymeric consisting of mannuronate (M)- and guluronate (G)-rich alginate, and hetero-
polymeric with different sequences of M and G (MG-blocks) [30, 23, 27].
3.3 Characteristic and properties of Alginate
3.3.1 Molecular weight
Alginates are polydisperse systems as a result of a broad range of composition, sequential
structure and consist of molecules of different molecular weight (MW). Due to this
property, the average molecular weight of alginate describes the average number of
molecule species in the whole distribution of the polymer [26, 22].
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Two most common ways to express the average molecular weight of a polymer is the
number average
___
nM and weight average
___
wM methods [26-27].
Alginate polymers are anionic (polymer is negatively charged) polyelectrolytes at pH 7
[31-32]. The molecular characterisations of polyelectrolytes are based on the Mark-
Houwink-Sakurada equation (intrinsic viscosity), membrane osmometry, sedimentation
equilibrium, gel permeation chromatography (GPC) and light-scattering measurement
[33, 26].
3.3.2 Solubility
Sodium-alginate is soluble in cold water while alginic acid and Ca-alginate are insoluble
[34]. This is important for encapsulation as it allows formation of beads during the
polymerisation reaction. Solubility of the polysaccharide depends on the pH, ion strength
and presence of divalent cations in the solute. pH determines the electrostatic charges on
the two uronic sugars [22, 30].
3.3.3 Gel formation
The primary functional property of the carbohydrate polymer is the ability to form gels in
the presence of multivalent or divalent cations such as Mg2+
< Ca2+
< Sr2+
< Br2+
[35].
Gelling properties of alginate depend on the ratio of the two uronic acids residual (M/G).
High G content and molecular weight will produce a strong less flexible gel with heat
resistant capability but prone to syneresis on freeze-thaw, whereas M rich alginates are
weaker but more flexible and can form gels either at very high or low Ca2+
concentration
[35]. Table 3.2 gives more information about the different M, G and MG fraction
composition of algal alginates. M/G ratio, molecular weight and viscosity influence the
physicochemical properties of alginate.
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TABLE 3.2 M, G AND MG FRACTION COMPOSITION OF COMMERCIAL AVAILABLE ALGAL ALGINATES [22]
SOURCE FG FM FMG
Laminaria japonica 0.35 0.65 0.17
Laminaria digitata 0.41 0.59 0.16
Laminaria
hyperborean
Leaf 0.55 0.45 0.17
Stipe 0.68 0.32 0.12
Outer cortex 0.75 0.25 0.09
Macrocystis pyrifera 0.39 0.61 0.23
Durviella Antarctica 0.29 0.71 0.14
Ascophyllum
nodosum
Fruiting body 0.10 0.90 0.06
Old tissue 0.36 0.64 0.20
Other valuable properties of alginates are swellability and film-forming, which are
important to biomedical applications [26]. This may cause the volume of the beads to
increase over time as water moves into the bead causing it to swell. Whether this has an
effect on function or growth is yet to be established.
3.3.4 Viscosity
In general, alginate solutions are pseudoplastic systems or non-Newtonian fluids.
Pseoudoplasticity refers to the decrease in viscosity of a solution with the increase of shear
rate (Figure 3.3). Temperature (Figure 3.4), molecular weight, concentration of the solution
(Figure 3.5) and pH may influence the viscosity. Autoclaving of alginate solution at 121°C
for 10 or 20mins can change the viscosity of the solution and probably causing changes in
the M/G chain length of the polymer and providing a less stable material for cell
encapsulation [22]. Lyophilisation (freeze drying) of alginate solution at the freezing
temperature can also effect the physical properties of polymer. During freeze-drying
operation, both “freezing and drying” stresses are produced which could alter the viscosity
of the polymer [36].
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FIGURE 3.3 VISCOSITY OF DIFFERENT ALGINATE CONCENTRATIONS VERSUS SHEAR RATE.
VISCOSITY OF THE SOLUTION DECREASES WITH INCREASING SHEAR RATE [30].
FIGURE 3.4 TEMPERATURE PROFILE OF THREE DIFFERENT 1% ALGINATE
SOLUTION VISCOSITY [30]
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FIGURE 3.5 SOLUTION CONCENTRATION EFFECTS ON THE POLYMER VISCOSITY [30]
The higher the concentration of the solution is, the greater its viscosity. During
encapsulation, cell media fluid mixtures pass through a 200µm nozzle thus surface force
increases. Higher concentrations of solution could results in non-spherical beads, which
alters the biocompatibility of the polymer providing a less suitable matrix for cells
development (Figure 3.5).
3.4 Purification Methods of Alginate for Clinical Use
Biomedical industry such as tissue engineering and cell transplantation is continuously
seeking biocompatible and non-toxic materials for cell encapsulation to be used in
bioartificial organs. Alginate hydrogels have been used as immobilisation matrix for
human and animal cells. Therefore, purification level of the biopolymer is crucial. During
harvesting and extraction of the biopolymer, it can be contaminated. Presence of various
impurities may initiate an immune response. Therefore, different purification methods have
been established but these unfortunately often resulting in changes to the viscosity of the
solution. As explained, successful encapsulation and maintenance of cell function and
growth through bead shape or morphology is affected by solution viscosity [2]. For this
reason a method is required that removes the presence of contaminants for regulatory
approval, without altering the chemical composition or viscosity.
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This section is concerned with the published insitu (clinical based) alginate purification
methods that aim to make the polymer suitable for human implantation. These processes
have significantly reduced endotoxins, proteins, polyphenols, ash and heavy metals from
alginates [26]. However, the methods were not primarily concerned with micron
particulate removal which affects the biocompatibility of the polysaccharide, as their
removal would have occurred along side removal of these other compounds. However, the
dramatic effects on the alginate composition and subsequent properties from these
processes made them unsuitable for Bioartificial Liver application. Therefore, this section
gives a brief overview of the different purification methods and their efficiency.
Firstly, it has become clear, after conducting a broad ranging literature review, that
currently there is no recognised standard purification method available for large scale
contamination free alginate production. Secondly, there are no medical standards that
would limit the concentration of impurities in the polymer. However, ATSM has published
„Standard and Guidelines for Biopolymers in Tissue-Engineered Medical Products; ASTM
Alginate and Chitosan Standard Guide‟. It states the major impurities of concern such as
endotoxin, protein, heavy metals and microbiological burden but it is limited only the
endotoxin level below 5 EU/kg of body weight [10] most of these components will be
removed insitu as part of the BAL quality assurance system, which is an inline filtration
system.
The first purification method was published in 1992 using free-flow electrophoresis (FFE).
FFE treatment contains two purification steps, a combined physicochemical pre-treatment
of alginate and a chemical purification procedure [19]. The FFE treatment is a complex,
time consuming, and expensive treatment. FFE method for purifying alginate endotoxin
and mitogenic contaminants level was successful, although the authors had pointed out that
“some unidentified residues were exhibited in the purified alginate after chemical
extraction” [19].
An alternative sodium alginate purification method, hollow fiber dead-end ultrafiltration,
was used by van de Ven, W. J. C. et al. [14] Membrane processes such as micro, nano and
ultra filtrations are utilised in drinking water treatment to remove visible materials and
substances with different particulate sizes [14].
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In 1997, De Vos, P. et al [18] published a report on „Improved biocompatibility but limited
graft survival after purification of alginate for microencapsulation of pancreatic islets‟. The
study focused on the correlation between the alginate purification methods and its impact
on the biocompatibility of the polymer microcapsules [18]. A multi – step (filtration,
extraction and precipitation) process was installed to purify raw sodium alginate, which
was filtered over four different pore sized filters (5.0, 1.2, 0.8 and 0.45µm). For removing
non-precipitated purities, Na-alginate solution was filtered over Buchner funnel three
times, and followed by a chloroform-butanol extraction step for the removal of the protein
content [18]. The final step was ethanol precipitation, which follows a Buchner funnel
filtration and at the end of the process, alginate is preserved by lyophilisation.
Biocompatibility of alginate capsules were improved after the multi-step purification but
graft abnormality and limited life-cycle was observed [18]. More details about the recently
published purification methods can be found in Appendix A.
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3.5 Fine Slow Sand Filtration Process
In drinking water treatment sand filtration (biological treatment), which is one of the oldest
water purification methods, is the fourth unit operation process in a water treatment plant.
Prior to this coagulation, flocculation and sedimentation remove large suspended
particulates and materials. Further removal of the particulate impurities is done by
percolating water through a permeable media (sand or anthracite) to remove fine
suspended particulates.
During the removal mechanism, suspended organic and inorganic materials are captured
within the pore spaces of the filter media, thereby removed from the water [37]. Numerous
factors affect the efficient operation of the filter media such as [38]:
Filter depth,
Grain size and sphericity (shape) of the filter,
Composition of the filter bed,
Filtration rate,
Influent concentration,
Characteristics of the suspended materials,
Water temperature, and
Porosity of the filter bed.
Fine sand filtration was chosen as an alternative purification method of Na-alginate
solution because the system is efficient in the removal of fine particles at low flow rate,
cost effective and easy to operate in comparison to the previous in house purification
methods (Section 3.4.).
In this chapter, the theory of sand filtration and flow of Newtonian and non-Newtonian
fluids is discussed.
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3.5.1 Physical parameters affect the operation of filter media
3.5.1.1 Shape of the filter media
Sphericity is defined as “the ratio of the equivalent hydraulic size (dh) to the sieve size
(geometric mean of passing and retaining sieve openings) (ds)”. It is a dimensionless value
and can be calculated by Eq. (3.1). Table 3.3. shows the calculated sphericity of filter
media by different researchers.
s
h
d
d
(3.1)
TABLE 3.3 SPHERICITY OF SAND
GRANULAR
MATERIAL
SPHERICITY RESEARCHERS
Sand 0.85 Ives, K. J.[39]
Sand 0.75-0.85 Tchobanoglous, G.
et.al [40]
3.5.1.2 Porosity of the bed
Porosity (n%) is defined as the ratio of the volume of voids to the total volume and
calculated from Eq. (3.2). The following parameters are required to calculate the porosity
of the granular material such as dry and wet weight of the media, depth of the media in the
filter column, and density of the media. As it can be seen from Table 3.4, several
researchers had determined the porosity of sand.
V
Vn v%
(3.2)
TABLE 3.4 POROSITY OF SAND
GRANULAR
MATERIAL
POROSITY
(n)
GRAIN
SHAPE RESEARCHERS
Sand 0.43 n/a Ives, K. J.[39]
Sand and grit 0.40-0.45 n/a Kézdi, Á.[41]
Sand 0.40-0.46 n/a Tchobanoglous, G.
et.al [40]
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3.5.2 Mechanism of filtration
The removal mechanism of fine suspended flocs from water by filtration through a
granular media is a complex process and can be classified as transport, attachment and
detachment mechanisms. Filtration can be further classified as surface (cake)- or depth
filtration but in all cases of filtration, laminar flow regime predominates [42].
Darcy‟s Law defines laminar flow of a fluid through permeable media (Figure 3.6).
FIGURE 3.6 HYDRAULICS OF A FLUID THROUGH PERMEABLE MEDIA [44, 51]
General equation Eq. (3.3) of his experiment (laminar flow condition) [45]
s
m
L
hAKQ
3
(3.3)
Where
Q flow rate [m3/s]
A cross section area of the column [m2]
Δh head loss of the column [m]
L length of the column [m]
K coefficient of permeability
L
hI
hydraulic gradient [dimensionless]
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“Permeability depends on the viscosity and the density of water, porosity, the size of the
pores, and the capillary forces between the medium and the liquid” [44].
Darcy’s Law
IkdL
dHk
A
Qqv ppa
(3.4)
Where
va approach- or filtration velocity [m/s]
kp permeability coefficient [m/s] [46]
I. The transport mechanisms during filtration
Straining or screening process takes place when the suspended particulates
percolating through a pore greater than the pore opening. This mechanism occurs
on the surface of the filter and is “independent of the filtration rate” [47].
Sedimentation: if the density of the particulates is greater than that of water they
will attached to the grain surface by gravitational force. Sedimentation is not
effective at removing particulates smaller than 1µm [47].
According to Camps, T. R. [48], settling behaviour of particles in suspension can be
classified as „free settling‟, „flocculent settling‟, „hindered (zone) settling‟ and
„compression settling‟ [48]. In accordance with the fine sand filtration experiment, it was
assumed that the settling is discrete and there is no interface among the sand particles [48].
During “the settling of discrete particles”, there are three flow regimes in a settling basin
e.g. laminar (10-4
<Re<1)-, transition (1<Re<104)- and turbulent flow (10
4<Re<10
6) (Figure
3.7) [48].
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FIGURE 3.7 DRAG COEFFICIENT (CD) FOR SPHERES AS A FUNCTION OF RE OVER LAMINAR-,
TRANSITION- AND TURBULENT FLOW REGIMES. IT CAN BE SEEN FROM THE FIGURE, THAT RE
INCREASES WITH DECREASING CD [48].
However, the value of Reynolds‟ number for permeable material under laminar flow is
Re<5 and can be calculated using Eq. (3.5).
tS
e
vdR
(3.5)
Where
Re Reynolds number [dimensionless]
µ dynamic viscosity of fluid [kg/ms]
ρ density of fluid [kg/m3]
vt terminal velocity [m/s]
dS sieve diameter [m]
During settling, three types of forces (gravitational force, buoyant force, and drag force)
affect the motion of a particle and drag occurs when water contacts with the surface of the
particle (Figure 3.8) [49].
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FIGURE 3.8 GRAVITATION FORCE (FG), BUOYANT FORCE (FB) AND DRAG FORCE (FD) AFFECT
THE MOTION OF A PARTICLE IN WATER DURING SEDIMENTATION [50]
Gravitation force is defined by Eq. (3.6)
gmFG ][N (3.6)
Where
g gravitational constant [m/s]
m mass of the particle [kg]
The buoyant force is given by Eq. (3.7)
S
OHB
gmF
2
(3.7)
Where
OH2 Density of water
3m
kg
S Density of particle
3m
kg
FD
FG
FB
PARTICLE
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The drag force is given by Newton‟s Law
2
2
2 vACF OHD
D
][N
(3.8)
Where
FD Drag force on particle [N]
CD Drag coefficient [dimensionless]
A Cross section area of the particle [m2]
vs settling or terminal velocity of the particle [m/s]
General equation for settling velocity is defined by the following Eq. (3.9)
]/[
3
4
2
2 smC
dgv
OHD
OHss
(3.9)
Figure 3.7 shows the three different flow regimes such as laminar, transition and turbulent.
Value of drag coefficient depends on the flow regime thus Reynolds‟s number.
Drag coefficient and settling velocity for Laminar flow 10-4
<Re<1 but for permeable
materials Re<5
e
DR
C24
(3.10)
Settling velocity for laminar fluid flow is defined by Stockes’ Law.
]/[
18
2
smdg
v ss
(3.11)
Where
g gravitational force [m/s2]
ρH2O density of the water [kg/m3]
ρs density of solid [kg/m3]
µH2O viscosity of the water [kg/ms]
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Camp‟s method for Transitional flow 1<Re<104 [49]
Drag coefficient form Eq. (3.9)
2
2
23
4
tOH
OHSD
v
dgC
(3.12)
Camp rearranged Eq. (3.12) to define
32
2
2
2
3
4
tOH
OHOHS
e v
g
R
Cd
(3.13)
and
OH
OHOHS
eD
dgRC
2
2
2
2
3
2
3
)(4
(3.14)
Camp‟s curves of eR
Cd and
2
eDRC versus Re can be found in Appendix B.
Inertial force: It can be seen from Figure 3.9 as flow lines approach the surface of
the filter grain the particle is forced to move out of the streamline [42]. “If the
particles have adequate inertia they maintain a trajectory” [42] therefore, they
deposit on the surface of the grain.
Diffusion (Brownian motion): natural source of water contains dissolved and
suspended solids. Suspended solids in water can be characterised as organic and
inorganic materials, bacteria, virus and other particulates. Particles with a particle
size greater than 1µm such as large colloids and soil can be removed during
filtration without additional chemical of physical treatment. Suspended particles
with a particle diameter less than 1µm are stable in the suspension and defined as
colloids.
Colloidal particulates can be further classified according to their affinity for water
such as hydrophobic and hydrophilic [37].
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FIGURE 3.9 TRANSPORT MECHANISMS DURING FILTRATION
THE MECHANISMS ARE: INTERCEPTION, INERTIA, GRAVITY, DIFFUSION, AND HYDRODYNAMIC
BY WHICH GRANULAR FILTER MEDIA REMOVE IMPURITIES FROM WATER [42]
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Three physical forces control the motion of colloidal particulates in water; namely,
electrostatic forces, van der Waals forces, and Brownian motion which is a random
movement of colloidal suspension [47].
Hydrodynamic action can be described in two ways. Firstly, when the shear field is
homogenous with a constant velocity gradient across the flow lines, spherical
particles will experience centrifugal force. As a consequence of this particles will
move across the shear field. Secondly, when the shear field is heterogeneous, as
on the filter pores, the particle will be diverted by the same force [32, 51].
II. Attachment mechanisms
1. Electrical double layer interaction: surface of a filter media, colloidal particles
and impurities are negatively (anionic) charged in water thus these materials
attract cationic ions, also known as “counter - ions” [37].
A stern layer around the electronegative particle is formed by counter ions such as
hydrogen. The second outer layer is the diffused layer where distribution of
cations and anions are presented but counter ions predominate. Combination of
the two outer layers is called the double layer [Figure 3.10]. As was mentioned
above, filter grain and impurities are negatively charged in water, thus the double
layer interaction will cause repulsion [37].
ELECTROSTATIC FIELD AROUND AN ANIONIC
PARTICLE
ILLUSTRATION OF ZETA POTENTIAL, SHEAR
PLANE, AND ELECTROSTATIC POTENTIAL
FIGURE 3.10 A, B ELECTRICAL DOUBLE LAYER [52]
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2. Van der Waals forces: the attraction or repulsion between atoms and molecules.
The magnitude of the force depends on the mass and the distance of the atoms and
molecules [52].
III. Detachment mechanisms
During the filtration cycle, suspended particulates are entrapped in the filter bed causing
reduction in the porosity. As a result of this, the head loss, filtration velocity, and the shear
force of the influent water thorough the porous media will be increased. At this point, the
filter bed becomes clogged and there will be a reduction in the filtration rate [37]. To
increase the filter performance, the porous media needs to be backwashed. During the
backwashing process, the colloidal particulates, which were entrapped among the grains,
become detached from the grains‟ surface [51].
3.5.3 Types of granular media filters
Granular media filters utilized in water treatment can be classified according to the filter
media type, filtration rate, driving force, and direction of flow [48]. In theory, sand filters
remove micro- and macro substances, and materials within the size spectrum of 1-1000µm
(Figure 3.11).
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FIGURE 3.11 DIFFERENT SEPARATION PROCESSES IN ACCORDANCE WITH THE SIZE DISTRIBUTION
OF POSSIBLE IMPURITIES PRESENT IN WATER [53]
GRANULAR MEDIA FILTRATION USED FOR REMOVING PARTICULATES OF SIZE RANGE BETWEEN
1.0µm-1000µm
Classification by filter media: There are three different filter media for the successful
operation of the filtration process such as single-, dual–, and multi-media (Figure 3.12).
Single medium filter consists of a layer of sand or anthracite whereas, dual medium filter
utilizes sand and crushed anthracite. The third filter type is the multi-media, which is a
triple layer of sand, crushed anthracite and garnet. The design parameters of different
media are shown in Table 3.5. A single medium filter removes macro particulates in the
range of 40-1000µm. Effective removal of micro particulates from water requires a dual-
or multi-media filter bed installation [54]. In theory, dual media filter (sand and anthracite)
are used in rapid filtration for micron particulate removal. For the filtration experiment fine
and coarse sand were used as dual media filter.
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FIGURE 3.12 DIFFERENT SAND FILTER MEDIA SYSTEMS
A), SINGLE MEDIUM FILTER (B) DUAL MEDIA FILTER, (C) MULTI-MEDIA FILTER [37]
Classification by filtration rate: filters can be slow (10 m3/m
2d)- or rapid (120 m
3/m
2d)
sand filters.
Classification by driving force: gravity or pressure filters.
Classification by direction of flow: downward flow or upward flow filters [37].
TABLE 3.5 DESIGN PARAMETERS OF SINGLE-MEDIUM, DUAL-, AND MULTI-MEDIA FILTERS [37]
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3.5.4 Hydraulics of sand filter
3.5.4.1 Head loss in clean filter
Throughout the operation of a clean filter under slow flow rate, suspended solids firstly
deposit in the top layers of the filter bed. Secondly, as the filtration time increases, the
suspended particles move deeper into the filter bed. As a result of this, head loss across the
filter will increase.
The Kozeny-Carman equation Eq. (3.15) describes the flow of clean water through a
permeable media when Re<10 [46]
2
3
26)1(
2
2
sOH
OHapproach
dg
vK
dL
dh
(3.15)
Where
Ψ Sphericity [dimensionless]
ε=n Porosity [%]
vapproach [m/s] can be calculated from the relation of volumetric low rate to cross
section area [46]
ds Diameter of the spheres [m]
K Permeability is a constant and range 4-5
OH2 viscosity of water at given temperature
sPa
sm
kg
OH2 density of water at given temperature
3m
kg
3.5.4.2 Filter backwashing
During continuous operation of uniform or stratified filter beds, suspended particles will be
entrapped among the pore spaces thus, reduction in porosity and increase in headloss
occurs. A clogged filter media state is formed and the system requires backwashing.
During backwashing, the upward fluid velocity expands the filter bed and causes
fluidisation.
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Hydraulics of expanded beds [46]
Determination of the expanded bed porosity using Fair – Hatch equation
22.0
t
ev
v
(3.16)
Where
εe porosity of expanded bed [%]
vt settling velocity of the particulates [m/s]
v approach velocity [m/s]
Depth of expanded bed
][
1
)1(22.0
m
v
v
LL
t
e
(3.17)
Where
L depth of filter bed [m]
Le depth of expanded bed [m]
Determination of minimum fluidisation velocity
e
sesmf
dgv
1180
)( 23
[m/s2]
(3.18)
Where
εe Porosity of the expanded filter bed
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3.5.5 Time-independent Non-Newtonian Fluids
Alginates have many industrial applications due to their chemical and physical properties
such as thickening and gelling. Notably, alginate solutions are time-independent,
pseudoplastic systems (non-Newtonian fluid) thus the viscosity of the solution depends on
concentration of the polymer, molecular weight, pressure, temperature, and rate of shear.
As stated, viscosity of such fluids depends on the concentration therefore, alginate
solutions can be further categorised as Newtonian or non-Newtonian fluids. In a published
article „Alginate-A Polysaccharide of Industrial Interest and Diverse Biological Functions‟,
Sabra, W et. al. [55] stated in accordance with other researchers, that rheologically a
medium viscosity, 0.5 % sodium alginate solution considered to be Newtonian fluid under
low (0.1-10 s-1
) and medium shear (10-1,000 s-1
) rates and time-independent under high
shear rate (1,000-100,000 s-1
). Whereas, rheologically a medium viscosity, 2.5 % aqueous
sodium alginate hydrocolloid is a non-Newtonian fluid at the end spectrum of low shear
rate range and high shear rate [55]. For cell encapsulation of living cells, viscosity of the
insoluble alginate gel is crucial because it affects the bead shape and resultant
microenvironment for cell growth and survival.
It is important to mention that non-Newtonian fluids can be subdivided into three groups
such as time-independent, time-dependent and viscoelastic fluids. In the next section
distinction between Newtonian and non-Newtonian fluids is presented.
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3.5.5.1 Viscosity of Newtonian fluids
Fluids behave differently under the application of external force (shear stress) and such
force causes continuous deformation, which can be defined as consistency. Consistency of
low molecular weightv liquids and gases at steady pressure and temperature is constant and
it is called viscosity. Viscosity of Newtonian fluids is independent of the applied rate of
shear and can be explained by the following Eq. (3.19) [56].
FIGURE 3.13 VISCOSITY OF NEWTONIAN FLUIDS [57]
][ sPadr
dv
(3.19)
Where
τ shear stress [Pa]
γ shear rate [s-1
]
r thickness of the fluid layer [m]
Correlation between shear stress and shear rate can be presented by flow curve, which is
linear for Newtonian fluid (Figure 3.14).
X
Y
dr
dv
Shearing force
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FIGURE 3.14 FLOW CURVE OF NEWTONIAN FLUIDS [57]
3.5.5.2 Viscosity of non-Newtonian fluids [57]
Solutions containing polymers of high molecular weighted are classified as non-Newtonian
fluids thus their “flow curve is non-linear” [57]. Four factors affect the viscosity of a non-
Newtonian (real) solution such as concentration, molecular weight, temperature, pressure
and shear rate. Further categorisation of real fluids:
“Time-independent non-Newtonian fluids” [57] (Bingham plastic, pseudoplastic and
dilatant fluids) (Figure 3.15)
FIGURE 3.15 FLOW CURVES OF VARIOUS TIME-INDEPENDENT NON-NEWTONIAN FLUIDS [57]
τ
γ
η=τ/γ
τ
γ
τB
Bingham (Plastic)
Dilatant
Newtonian
Pseudoplastic
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a) Bingham plastic
As can be seen from Figure 3.15, flow curve of a Bingham plastic fluid is a
straight line and τB is given by the intersection on the shear stress axis [57].
Rheological properties of a Bingham plastic fluid is described by the
following Eq. (3.20)
][PaB (3.20)
Where
τ shear stress [Pa]
τB Yield stress [Pa]
γ shear rate [1/s]
b) Pseudoplastic fluids: viscosity of these liquids decrease with increasing
shear rate. Flow curve of these fluids is slightly convex (Figure 3.15).
Ostwald (power law) is used for describing the rheological properties of the
fluid [57].
][)( Pak n (3.21)
Where
τ shear stress [Pa]
γ shear rate [s-1
]
k consistency index, [55]
n flow behaviour index, for pseudoplastic fluids between 1 to 0 [55]
Important to note, “k depends on temperature and measures the consistency of the fluid.
The higher “k” the more viscous the fluid”, n measures the degree of non-Newtonian
behaviour [57].
c) Dilatant fluid: viscosity of the solution increases by increasing shear rate.
A 0.2%, alginate solution may be considered to be a Newtonian liquid as the low
concentration produces more water like properties [55], therefore further analysis will be
carried out to determine the Newtonian or non-Newtonian fluid dynamics behaviour of Na-
alginate solution having different concentration.
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4 MATERIAL AND METHODS
The major objective of the present work was to investigate the use of fine sand filtration as
an alternative purification method for particulate removal from Na-alginate. This section
includes:
purification of Na-alginate by sand filtration, a method for large scale
production,
in vitro analytical methods analysis of purity of alginate,
description of the experimental work,
equipments and materials are presented (Figure 4.1),
fine sand filtration experiments.
The alginate used was research grade, medium viscosity sodium alginate (Sigma-Aldrich
UK) with the following specification: viscosity of 2% at 25°C approximately 3500cps and
molecular weight of alginic acid sodium salt range between 80,000-120,000. Granular
media (RH-70 and RH-110) were supplied by Sibelco UK Ltd.
FIGURE 4.1 LIFE CYCLE OF THE EXPERIMENTAL WORK
The experimental work was divided into four stages:
Stage I. Fine sand filtration with the aim of removing macro particulates from research
grade Na-alginate;
Stage II. Lyophilisation 0.2% filtered alginate solution is shell frozen in a dry ice acetone
bath in 1L round bottomed flasks, to be lyophilised to sublimate water, leaving dry alginic
acid salt.
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Stage III. Reconstitution of alginate to final concentration of 1.0%, 1.25%, 1.5%, 1.75%,
1.875% and 2%, and autoclaving for 10 mins at 121°C.
Stage IV. HepG2 cell encapsulation preparation of 1.875% alginate beads containing a
liver cell line using Inotech microencapsulator.
4.1 Preparation of 2% HEPES buffered alginate solution
To make 2% sodium alginate solution, 8.76 g NaCl was dissolved in Milli-Q water under
constant stirring, than 15 ml 1M HEPES (Sigma-Aldrich UK), bringing to pH7.4 using
NaOH. The saline solution was placed in a foil covered bottle. Na-alginate powder (20g),
was gradually added to the saline solution allowing to dissolve and stirred overnight by a
mechanical stirrer [58]. For the filtration test, 2% aqueous Na-alginate solution was diluted
to 1:10 in Milli-Q water and filtered through sand.
Milli-Q water is produced by Millipore; Milli-Q(R)
Integral water purification system. The
four cartridges remove microorganism, ionic and organic contaminants and subsequently
the water is filtered through Millipak Express 0.22 µm membrane filter thus, the system
provides fine suspended material and bacterial free ultra pure water for laboratory use
(Table 4.1) [59].
TABLE 4.1 WATER QUALITY PARAMETERS OF MILLI-Q WATER [59]
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4.2 Testing of filter media
Filtration media tests were conducted to achieve purification of sodium alginate solution.
Two different granular materials were used as filter media (RH-70 and RH-110).
4.2.1 Chemical analysis of filter media
The aim of the analysis was to determine the chemical composition of the granular filter
media, which are 99% silica sand. The examination was done by SIBELCO UK Ltd
(Appendix C).
4.2.2 Physical analysis of filter media
4.2.2.1 Grain size distribution analysis
The aim of the sieve analysis is to assess the particle distribution of sediments, to
determine the particle sizes and to evaluate the cumulative percent passing of the granular
material. Grain size distribution was done by sieve analysis. Results of the analysis are
presented in the particle distribution graph (Appendix D), which is a semilogarithmic
graph, where the X axis (logarithmic scaled) shows particle size and the Y axis (linear
scaled) % passing of the sediment. Another important parameter, the uniformity coefficient,
that is a ratio between 60%- and 10% of granular materials passing Eq. (4.1), is also
determined during the analysis.
Uniformity coefficient
10
60
d
dU
(4.1)
Where
d10 also know as effective grain size (deff)
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4.2.2.2 Density of sands
The density of granular material is required for the calculation of settling velocity of the
particulates, and determination of headloss through the filter bed. In theory, the test is
carried out in a density bottle [39]. Density of filter medium was evaluated by SIBELCO
UK Ltd. hence density of RH-70 was 2,650 kg/m3 and assumption was made for the
density of RH-110. Assumption analysis is described in more details in Section 5.1.1.2.
4.2.3 Settling velocity of individual grains
There are two main reasons to determine the “settling velocity of individual grains of
uniform size in water of known temperature” [39]. Firstly, during backwashing in a “water
alone” system, it is establishes the “stratification behaviour” of the grains. Secondly, the
hydraulic diameter can be calculated and later the sphericity of the grains can be
determined [39]. In theory, settling velocity is determined based on the average time
required to settle 20 individual wet sediment grains (sand or anthracite) in a 1 m column at
a known water temperature.
4.2.4 Shape (sphericity) of filter media
The settling velocity can be used to determine the shape of the filter grains using the Eq.
(4.2) [39]. Sphericity of filter media was determined by SIBELCO Ltd thus grain shapes
are sub-angular and sphericity medium (Appendix D).
s
h
d
d
(4.2)
Where
Ψ sphericity [dimensionless],
Ψ=1 the grain is sphere,
Ψ<1 the grain is non-sphere [39].
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4.2.5 Porosity of filter media
Porosity of the RH-110 filter bed was determined using Eq. (3.2) and an assumption was
made for RH-70 based on literature. Dry and wet weight of the medium and depth of the
medium in the filter column were measured, and density of the sands was calculated.
4.2.6 Determination of headloss in clean granular media filter
4.2.6.1 Flow of non-Newtonian alginate fluid in porous media
For the filtration experiment a 2% sodium-alginate solution was prepared and was diluted
to 1:10 ratio with Milli-Q water. As a result of this, the following assumptions were made
and based on Sabra, W. et al. [55] and Cancela, M. A. et al. [60]:
a 0.2%, medium viscosity Na-alginate solution is considered as a Newtonian fluid
between low and medium shear rate ranges,
the viscosity of the fluid depends on temperature and shear rate,
flow regime is laminar,
flow of the fluid through porous media is described by Darcy‟s Law.
Headloss development in the permeable media, flow rate, and filtration rate calculations
are based on the above stated assumptions and the results are presented in Chapter 5.
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4.3 Systems preparation for filtration
4.3.1 Treatment of filter media before use
Acid treatment was used to eliminate the micronutrient impurities from the sand. The sands
used in the experiment were washed with 20% hydrochloric acid (HCl) and left overnight.
HCl was supplied by Fisher Scientific UK Ltd with the following specification: analytical
reagent grade 32% HCl, Code H/1100/PB17, Batch 0929448. After acid bath, the granular
materials were mechanically stirred and rinsed in Milli-Q water several times, gradually
increasing the pH to 7.
4.3.2 Treatment of the filtration systems before use
Glass tubes were autoclaved for 15 min at 121°C, and due to the construction material
(PVC) of the large scale system, the filter tube was washed by a 70% Methanol/H2O.
4.4 Filtration systems installation
Particular objectives of the research project were to determine the most effective granular
media filter and flow rate for micron particulate removal. Therefore, filtration tests (single
medium and dual media filters) were run and the process operation was subdivided into
five phases. Technical parameters of the small scale systems were the same in Phase I-III.
Phase I. Aim was to determine the most efficient granular filter medium size.
Technical parameters of the small scale systems:
• Two glass tube were used for the test (Figure 4.2),
• d(external)=0.018m of the tube,
• d(internal)=0.0143m of the tube,
• Height (H) = 0.40m of the tube.
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FIGURE 4.2 PHASE I. FILTRATION: SMALL SCALE SYSTEM BEFORE THE FILTER MEDIA
INSTALLATION
Parameters of the small scale filtration systems:
Uniform filter medium RH-70 and RH-110,
Filter media depth in both columns 0.25m,
Variable flow rates were tested for the efficient operation of the filtration system.
Phase II. The aim of this phase was to establish the most suitable flow rate according to
the removal efficiency. Technical parameters of the small scale system and the filtration
system are the same as in Phase I.
Phase III. The aim of this phase was to specify the most efficient filter medium depth.
Parameter of the small scale filtration system:
Uniform filter bed of RH-70 and RH-110,
Filter media depth in both columns 0.30m,
Variable flow rates.
Sand
RH-110
Sand
RH-70
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Phase IV. For the more efficient removal of macro particulates a dual-media filter was
introduced at the small scale system. A large scale (Figure 4.3) single media filter was also
set up with the aim of comparing the filtration results such as flow rate and particulate
removal efficiency to the performance of small scale systems.
Technical parameters of the small scale systems were the same as in Phase I-III.
Technical parameters of the large scale system (Appendix E):
• PVC built filter tube,
• d(external)=0.06m of the tube,
• d(internal)=0.0465m of the tube,
• Height (H) = 1.25m of the tube.
Parameters of the large scale filtration system:
• Mono (single) medium filter of RH-110,
• Filter medium depth 0.6m.
Parameters of the small scale filtration system (Figure 4.4):
• Dual media filter combination of RH-70 and RH-110,
• Total depth of the dual media filter was 0.30m (RH-70=0.13m and RH-110=0.17m)
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FIGURE 4.3 PHASE IV. FILTRATION: LARGE SCALE, SINGLE MEDIA FILTRATION SYSTEM
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FIGURE 4.4 PHASE IV. FILTRATION: DUAL MEDIA FILTRATION SYSTEM
Phase V. Due to an unforeseen technical problem, which contaminated the effluent during
the single media filter operation, both systems in Phase IV. were shut down on 9th
July
2009. Contamination caused turbidity in the effluent and gave a „yellowish‟ colour for the
filtered 0.2% sodium-alginate solution. Thus, Phase V. is repetition of Phase IV.
Problem statement
Cleaning technique of the single media was insufficient therefore, the filtered sodium
alginate was contaminated. The possible reasons for the contamination were
Filter media was sitting in acid bath overnight rather than continuously stirred,
Sand might be contaminated by microorganisms.
Dual-media filter (DMF)
combination of:
RH-70 (13cm)
RH-110 (17cm)
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Problem Solving
As a consequence of the above, the following problem solving steps were applied. Firstly,
a new sterilisation technique of the single medium was conducted. Sand was washed in
20% HCl solution overnight to remove biological material. After acid bath, the granular
materials were mechanically agitated and rinsed in Milli-Q water several times, gradually
increasing the pH to 7. Finally, the sand was autoclaved for 15mins at 121°C.
Secondly, to make sure that the effluent purity level was adequate water samples were
taken and turbidity level was measured. Thirdly, the filter bed was backwashed because the
turbidity level of the first sample was too high (102.4 NTU). Milli-Q water (0.3 NTU) was
used as control sample for monitoring the effluent turbidity concentration. Following
backwashing the turbidity was reduced to 2.4 NTU, which is higher than Milli-Q water but
significantly lower than before. This may be a reason for potential of added material to the
alginate during filtration.
Parameters of the large scale filtration system:
• Mono (single) medium filter of RH-110,
• Filter medium depth 0.8m.
Parameters of the small scale filtration system (Figure 4.4):
• Dual media filter combination of RH-70 and RH-110,
• Determination of depth of the filter bed is explained in Chapter 5.
In brief, the total depth of the dual media filter was 0.30 m (RH-70=0.13m and
RH-110=0.17m)
4.5 Sand filtration experiment
Before each filtration test fresh 2% HEPES buffered sodium alginate solution was prepared
which was highly viscous, and therefore diluted to 1:10 ratio in Milli-Q water. The alginate
solution was prepared one day priori to treatment. Gravity was used as driving force for the
filtration and the volume of the filtration tank was 10L. Sand filtration was operating with
constant inflow.
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4.5.1 Filtered aqueous sodium-alginate samples
Filtration experiments were run overnight and control samples were taken before filtration
for further analysis. Filtered aqueous Na-alginate samples were collected on the following
day and immediately lyophilised. Table 4.2 shows the collected filtered sodium alginate
samples during the fine sand filtration periods.
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TABLE 4.2 FILTERED NA-ALGINATE SAMPLES DURING THE FINE SAND FILTRATION PERIODS
FILTRATION TEST
FILTRATION PERIOD FILTRATION
TIME (DAY)
VOLUME OF THE
FILTERED SAMPLE
(ml) STARTED FINISHED
PHASE I.-II. FILTRATION
SA
MP
LE
CO
DE
RH-70/I. 4.30pm
16th June 09
9am
17th June 09 0.90 332
RH-70/II. 9am
17th June 09
5.15pm
17th June 09
0.34 182
RH-70/III. 5.15pm
17th June 09
9.30am
18th June 09 0.68 275
RH-70/IV. 9.30 am
18/06/09
5.15pm
18/06/09 0.36 250
RH-70/V. 5.15pm
18/06/09
12.40 pm
19/06/09 0.83 442
RH-110/I. 4.30pm
16th June 09
9am
17th June 09 0.90 250
RH-110/II. 9am
17th June 09
5.15pm
17th June 09 0.34 136
RH-110/III. 5.15pm
17th June 09
9.30am
18th June 09 0.68 255
RH-110/IV. 9.30 am
18/06/09
5.15pm
18/06/09 0.36 244
RH-110/V. 5.15pm
18/06/09
12.40 pm
19/06/09
0.83 332
SA
MP
LE
CO
DE
RH-70/VI. 4.20pm
30/06/09
9.45am
01/07/09 0.73
275
RH-70/VII. 9am
01/07/09
9.30am
02/07/09 1.02
525
RH-110/VI. 4.20pm
30/06/09
9.45am
01/07/09 0.73
275
RH-110/VII. 9am
01/07/09
9.30am
02/07/09 1.02
525
PHASE IV. FILTRATION (THE SYSTEM WAS SHUT DOWN ON 09/07/09)
SA
MP
LE
CO
DE
DMF-I. 5pm
07/07/09
10am
08/07/09 0.71 500
DMF-II. 10am
08/07/09
12.40pm
08/07/09
0.11 230
MMF-I. 6pm
07/07/09
10am
08/07/09
0.67 500
MMF-II. 10am
08/07/09
12.40pm
08/07/09
0.11 500
PHASE V. FILTRATION
SA
MP
LE
CO
DE
DMF-III. 2.30pm
21/07/09
11.20am
22/07/09 0.45 285
DMF-IV. 11.20am
22/07/09 Filter bed was clogged. 176
MMF-III. 6pm
21/07/09
10am
22/07/09 0.33 490
MMF-IV. 6pm
22/07/09
9am
23/07/09 0.62 520
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TIMEA GREGO 43
4.5.2 Sodium alginate viscosity measurement
Viscosity of the sodium alginate solutions was measured to verify the rheological
properties of the fluid. The dynamic viscosity of the alginate solutions having different
concentration, autoclaved and non-autoclaved, fresh and old samples were measured using
Bohline CVO 100 Analogue RSO Viscometer. Samples were dissolved in Milli-Q water
and viscosity measurements were made at 25°C.
Na-alginate powder, with medium viscosity of 2% at 25°C approximately 3500cps. The
Molecular weight of alginic acid Na-salt ranged between 80,000-120,000 (as specified by
the manufacturer). According to this information, viscosity of a 2% Na-alginate solution
could be calculated.
sPaPcps 32 10101 smkgsPa /][
Therefore viscosity of 2% sodium alginate solution at 25°C is smkgcps /5.3500,3 .
4.5.3 Turbidity
It was described previously, during the single medium filter operation the effluent water
was contaminated, hence filter backwashing was performed. This approach, which is part
of rapid filtration, was used to clean the filter bed and to remove much of the impurities,
which were entrapped among the pores. Filter backwashing had been running for 35 mins
and, as a result, turbidity level of the effluent was reduced from the initial concentration of
102.5 Nephelometric Turbidity Units (NTU) to 2.4 NTU. Turbidity was measured in HACH
Ratio/XR Turbidity meter, USA.
4.6 Lyophilisation of filtered sodium-alginate
Lyophilisation or freeze – drying, which is the second stage during the experiment life-
cycle (Figure 4.1), is a method by which filtered sodium-alginate solution is frozen and
then water is removed by sublimation. Freeze-drying process has become a standard
operation process in the medical field for providing “stable state” for liquid materials [61].
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Lyophilisation of the solution involves the following steps:
a. Shell freezing of filtered sodium alginate solution: 1L round-bottomed flasks
were manually spun in an acetone bath, which was cooled below 0°C by dry ice.
During this process, a slim layer of frozen sodium alginate formed around the
internal wall of the flask (Figure 4.5). The samples were kept in a freezer to prevent
melting of alginate before they could be transferred to the vacuum.
FIGURE 4.5 SHELL FREEZING PROCESS OF FILTERED NA-ALGINATE SOLUTION
b. Drying of the frozen alginate under vacuum: the sample was placed under a
vacuum and placed in circuit with a freezer at -40°C, where water sublimed to the
freezer section and giving the end product of dry alginic acid (Figure 4.6).
FIGURE 4.6 DRIED ALGINIC ACID AFTER LYOPLISIATION
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4.7 Reconstruction of sodium-alginate
At the third stage of the experimental work (Figure 4.1) dried sodium alginates were
rehydrated at ambient temperature in Milli-Q water to a final 1.0%, 1.25%, 1.5%, 1.75%,
1.875% and 2% solution under constant stirring. Therefore, the most appropriate
concentration could be chosen for immobilisation of HepG2 cells in alginate matrix. In
additional to this, to improve the accuracy of particulate analysis the samples were
centrifuged.
4.7.1 Analytical centrifugation
22 samples (Table 4.2) were prepared for two separate centrifuge runs. Dry Na-alginates
samples were dissolved in 1ml Milli-Q water to a final 2% solution under constant
agitation, and then centrifuged for 100mins at 16,000 relative centrifugal force (rcf). “x g”
is the unit of rcf and “g” presents the force of gravity. After the first centrifugation
supernatants were removed from pellet, and resuspended in 1ml Milli-Q water and the tube
was filled up to 1.5ml and centrifuged again as before. At the end of the second
centrifugation, supernatant was taken off and resuspended in 250µl Milli-Q water.
FIGURE 4.7 ANALYTICAL CENTRIFUGE ANALYSIS BY EPPENDORF CENTRIFUGE 5415R
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4.7.2 Determination of the size distribution of the particulates
Particle size distribution of filtered, 2% Na-alginate solutions were determined by a
NIKON Eclipse TE200 light microscope. After centrifugation the samples were placed
onto glass microscope slides and to prevent the alginate droplets drying out the samples
were covered with a protective glass sheet and the mean particle size distributions were
calculated. Particle counting of filtered solutions were done by PAMAS SBSS Liquid
particle counting system with the aim of determining size ranges and quantities of the
particles by light obscuration.
4.7.3 Encapsulation of filtered sodium-alginate
Due to lack of experience in cells encapsulation, the empty alginate beads and
immobilisation of HepG2 cells in alginate matrix were done by Amir Gander and assisted
by Timea Grego.
4.7.3.1 Encapsulation of filtered sodium alginate
The aim of the empty beads encapsulation was to analyse the morphology of the beads
thus, filtered, final 1.0%, 1.25, 1.5%, 1.75%, 1.875% and 2% concentration of Na-alginate
solutions were prepared in Milli-Q water, and autoclaved at 121°C for 10 mins. A 50:50
ratio alginate was mixed with high glucose complete media solution, and applied into a
syringe, which was connected to Inotech encapsulation system, which is a droplet
generator utilising vibration [63]. Alginate and media mix passed through a 200µm nozzle
under constant electromagnetic vibration causing bead formation. Polymerisation of the
alginate matrix occurs when the droplets fall into the polymerisation buffer in a 204 mM
CaCl2, 150 mM NaCl and 15 mM HEPES buffer solution (pH 7.4) and had been stirred for
10mins. Then, the beads were washed in Alpha MEM media (Invitrogen) and resuspended
in PBS + Ca2+
(Lonza) [63].
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4.8 Encapsulation of HepG2 cells
A 20 ml filtered sodium-alginate with a final concentration of 1.875% was prepared in
Milli-Q water. HepG2 cells were cultured in monolayer for four days, then harvested by
trypsinisation and added to a 50:50 alginate to media mix at 1x106/ml beads. Alginate and
cell-media mix were passed through the 200 µm nozzle of the Inotech encapsulator
creating alginate-HepG2 beads upon immersion into the polymerisation buffer containing
Ca2+
for 10 mins [63].
4.8.1.1 Morphology of empty beads and cell cultured alginate beads
Morphology of the beads was analysed by NIKON Eclipse TE200 microscope. Empty and
HepG2 containing alginate beads were placed on a microscope slide and photographs were
captured.
4.8.1.2 Determination of cells viability in beads
For the live and dead quantitative analysis, “alginate beads were mixed in medium and
transferred from the culture vessel to a 1.5ml microfuge tube. The beads were left to settle
and the volume of the beads was adjusted to 200µl. After this, a 200µl sample of HepG2
alginate microcapsules was washed twice and re-suspended in 500µl of PBSCa+Mg
”. To
identify the viability of the encapsulated cells, “20µl of 1mg/ml propidium iodide (PI) dead
dye” and for the non-viability analysis “10µl of flourescein diacetate (FDA) live dye was
added and incubated for 90seconds, than the tubes were mixed gently”. “The beads were
washed with PBSCa+Mg
again and finally resuspended in 0.5ml of PBSCa+Mg”
. The dyed
microcapsules were placed on a microscope slide for image analysis “using an excitation
filter of 510-560ηm and an emission filter of 590ηm for PI dyed cells, and for FDA dyed
cells, and an excitation filter of 465-495ηm and an emission filter of 515-55ηm. Digital
images were captured with NIKON Eclipse TE200 microscope and the built in DX1200
camera and utilising Lucia imaging software package” [62].
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5 EXPERIMENTAL RESULTS AND DISCUSSION
Fine sand filtration was investigated as a possible purification method for purifying
research grade sodium-alginate on a large scale for clinical use. In this section, results of
the filter media test, viscosity measurement, empty beads and HepG2 cell encapsulation in
purified Na-alginate are presented and discussed.
5.1 Testing of filter media
Physical and chemical analysis of the filter media and the various filter tests were
undertaken to determine its suitability for fine sand filtration. In the following sections, the
results of the analysis are presented and discussed in more details.
5.1.1 Physical analysis of filter media
5.1.1.1 Grain size distribution analysis
The aim of the granulometric analysis, which was conducted by SIBELCO UK Ltd, was to
determine the effective grain size and uniformity coefficient of the filter media. Not just
the previously mentioned parameters, but also the fine and very fine particles size
distribution were determined. It is important to know the distribution of these fractions
because these granular materials have large specific surface area, and their surface charge
(zeta potential) is unequal, therefore during sorption these particles present large surface
activity.
The value of the particle diameter at which 60% and 10% of the sands is finer was read
from the graphs. Therefore, uniformity coefficient and effective size range were
determined. In accordance with the sieve analysis, RH-70 was considered as coarse sand
with U=1.6 and deff=135µm, whereas RH-110 was fine sand with U=1.7 and deff=82µm.
Table 5.1 shows the reduced data of grain size distribution analysis of coarse and fine sand
such as cumulative passing and retained fractions of the media and classification of
sediments. Figure 5.1 and 5.2 shows the grain size distribution graphs of coarse and fine
sand. As can be seen from the graphs, the more steep a graph, the more uniform the
particulate distribution.
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TABLE 5.1 REDUCED DATA OF GRAIN SIZE DISTRIBUTION ANALYSIS OF
RH-70 (COARSE SAND) AND RH-110 (FINE SAND)
BS STANDARD SIEVE
NOMINAL APERTURES
(µm)
MESH
NUMBERS
PASSING
(%)
RETAINED
(%)
CUMULATIVE
RETAINED (%)
SEDIMENT
CATEGORIES
RH-70 (COARSE SAND)
710 22 100.00 0.00 0.20 Coarse sand
500 30 99.80 0.20
355 44 96.90 2.90 23.10 Medium sand
250 60 76.70 20.20
180 85 33.80 42.90 69.00 Fine sand
125 120 7.70 26.10
90 170 2.30 5.40 7.00
Very fine
sand 63 240 7.70 1.60
<63 240-440 0.00 0.70 0.70 Slit/Clay
RH-110 (FINE SAND)
355 44 100.00 0.00 0.20 Medium sand
250 60 99.80 0.20
180 85 89.10 10.70 59.00 Fine sand
125 120 40.80 48.30
90 170 15.20 25.60 37.10
Very fine
sand 63 240 3.70 11.50
<63 240-440 0.00 3.70 3.70 Slit/Clay
FIGURE. 5.1 GRAIN SIZE DISTRIBUTION GRAPH OF RH-70
PARTICLE SIZES (µm) VERSUS CUMULATIVE PASSING OF THE GRAINS (%)
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FIGURE. 5.2 GRAIN SIZE DISTRIBUTION GRAPH OF RH-110
PARTICLE SIZE (µm) VERSUS CUMULATIVE PASSING OF THE PARTICLES
5.1.1.2 Density of sands
SIBLECO UK Ltd could only determine the density of RH-70 (Appendix D) and an
assumption was made for RH-110 which was based on literature [39-41, 58]
(Table 5.2). As a consequence of the above mentioned, density of granular media is
ρ=2,650kg/m3.
TABLE 5.2 DETERMINED DENSITY OF RH-70 FILTER MEDIUM COMPARED TO DATA AVAILABLE IN
LITERATURE
SEDIMENTS DENSITY (kg/m3) RESEARCHERS
Quartz sand 2,650 Ives, K. J. (1990) [39]
Sand and grit 2,400-2,600 Judd (2006) [58]
Sand and grit 2,650 Kézdi, Á. (1969) [41]
Sand 2,550-2,650 Tchobanoglous, G. et.al
[40]
RH-70 (Moist)
Sand
2,650 SIBELCO UK Ltd.
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TIMEA GREGO 51
5.1.2 Sphericity (shape) of filter media
According to physical analysis of the filter media, grain shape of RH-70 and RH-110 was
sub-angular with medium sphericity (Appendix D). Moreover, two charts of sphericity and
roundness were provided by SIBELCO UK Ltd., and as can been seen from the charts the
more rounded a grain, the higher the sphericity (Ψ) value (Appendix F). In accordance
with the charts, the shape of filter media is non-spherical and the estimated value of
sphericity (0.78) was based on the provided charts and literature (Table 5.3).
TABLE 5.3 ESTIMATED SPHERICITY OF RH-70 AND RH-110 COMPARED TO DATA AVAILABLE IN
LITERATURE
GRANULOMETRIC
MATERIAL
SPHERICITY GRAIN SHAPE RESEARCHERS
Sand 0.85 n/a Ives, K. J. (1990)
[39]
Sand 0.75-0.85 n/a Tchobanoglous, G.
et.al [40]
RH-70 and
RH-110 (Moist)
Sands 0.78
(a) Sub-angular
SIBELCO UK Ltd.
and (a) Casey [46]
5.1.3 Settling velocity of individual grains
The settling velocity of 20 individual coarse and fine sand grains settling through 1 m
column at water temperature 20°C (Appendix G) was measured and the average settling
velocity was calculated (Table 5.4).
TABLE 5.4 AVERAGE SETTLING VELOCITY OF COARSE AND FINE SAND GRAINS
GRANULAR MATERIAL AVERAGE SETTLING VELOCITY
vav (m/s)
RH-70 (COARSE) 0.05
RH-110 (FINE) 0.03
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5.1.4 Porosity of filter media
In this section, porosity calculation of RH-110 (fine sand) is presented. As can be seen
from Table 5.3 and Table 5.5, there is a correlation between porosity and sphericity of the
sediments thus, the higher sphericity value, the lower the porosity. According to the
physical analysis of the filter media, grains shape is sub-angular. Therefore, Table 5.5
shows the assumed porosity of filter media based on literature review.
TABLE 5.5 ESTIMATED POROSITY OF RH-70 AND RH-110
TYPE OF GRANULAR
MATERIALS
POROSITY
(n)
GRAIN
SHAPE
RESEARCHERS
Sand 0.43
n/a Ives, K. J. (1990, p
144.) [39]
Sand and grit 0.40-0.45
n/a Kézdi, Á. (1969, p 48.)
[41]
Sand 0.40-0.46
n/a Tchobanoglous, G.
et.al [40]
RH-70 and
RH-110 (Moist) Sand 0.43(a)
Sub-
angular
SIBELCO UK Ltd
(a) Casey [46]
research.
Porosity of RH-110
In this part, the porosity (n) and void ratio (e) of the single (RH-110) medium filter, water
content (w), specific volume (V) had been determined.
Mass of the wet sand (RH-110) Gw=2.80kg
Mass of the dry sand (RH-110) Go=2.08kg
Depth of the mono media filter (MMF) HMMF=0.8m
Internal diameter of the filter tube DMMF=0.0465m
Density of the sand (assumption) 3/2650 mkgs
Density of the sand was adopted from Kézdy, Á. and Ives, K. [39, 41]
Temperature during filter operation T=20°C
Single medium filter is a complex system and can be divided into three parts i.e. air, water
and solids (Figure 5.3).
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FIGURE 5.3 MASS –VOLUME RELATIONSHIP OF A SEDIMENT SAMPLE [51]
Volume related symbols [64]
V=Vs+Vv Total volume of the sand
Va Volume of the air
Vv=Va+VW Volume of the voids
Vs Volume of the solids
Vw Volume of the water
Mass related symbols [64]
M=Mw+Ms Total mass of sand sample
Ma Mass of air (0)
Ms Mass of solids
Mw Mass of water
STEP 1 Determination the total volume of the sand
33222
1036.18.04
14.30465.0
4
14.3
4mxm
mH
Dh
dV MMF
MMF
(5.1)
STEP 2 Calculation of water content (w%)
%6.3410008.2
08.280.2100%
0
0
kg
kgkg
G
GGw n (5.2)
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TIMEA GREGO 54
STEP 3 Volume of solids (Vs)
34
3
0 1085.7/2650
08.2mx
mkg
kgGV
s
s
(5.3)
STEP 4 Volume of voids (Vv)
343433 1075.51085.71036.1 mxmxmxVVV sv
(5.4)
STEP 5 Void ratio (e)
732.01085.7
1075.534
34
mx
mx
V
Ve
s
v (5.5)
STEP 6 Porosity (n%) of RH-110
%2.421001036.1
1075.5100
33
34
mx
mx
V
Vn v (5.6)
Comparing the calculated porosity value to the estimated porosity based on the literature
(Table 5.5), it can be see that porosity of RH-110 was a little bit over 42% and close to
43%. Thus, the calculated and assumed sphericity (Table 5.3) are valid.
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5.2 Hydraulic of filtration
As was described previously, a 0.2%, medium viscosity sodium-alginate solution was
considered as a Newtonian fluid between low and medium shear rate ranges. Viscosity
measurements were conducted to determine the rheological properties of Na-alginate
solutions having different concentration and to validate the above stated assumption. As a
result of this, a 0.2%, medium viscosity Na-alginate solution is Newtonian fluid. In
section 5.3, the results of the viscosity measurements are discussed in more details. In
accordance with the above, head loss in clean water and during backwashing, volumetric
flow rates, and filtration rate calculations were determined.
Firstly, it was necessary to determine the effective size, and the uniformity coefficient of
the granular filter media. These values were obtained from the sieve analysis and presented
in Table 5.6. Secondly, the headloss in the clean filter bed was calculated. Detailed
calculation of hydraulic of filtration can be found (Appendix H).
TABLE 5.6 PHYSICAL PARAMETERS OF THE FILTER MEDIA
PHYSICAL PARAMETER SYMBOL UNIT RH-70 RH-110
SPHERICITY Ψ dimensionless 0.78 0.78
POROSITY n dimensionless 0.43 0.422
OPERATIONAL
TEMPERATURE
T °C 20 20
UNIFORMITY COEFFICIENT 10
60
d
dU
dimensionless 1.6 1.7
EFFECTIVE SIZE d10 µm 135 82
GEOMETRIC MEAN OF
AVERAGE SIEVES ds
m 1.77x10-4
1.04x10-4
AVERAGE SETTLING
VELOCITY vs
m/s 0.05 0.03
5.2.1 Determination flow regimes and drag coefficient
STEP 1. Determination of the value of Reynolds‟ number (Re) for coarse and fine sands
using Eq. (3.5)
RH-70
9
)/100087.1(
)/05.0()/23.998()/1077.1(3
34
2
2
mskg
smmkgsmvdR
OH
OHse
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RH-110
As can be seen from the results, the flow region of coarse sand grains was transition and
fine sand grains was laminar.
STEP 2. Determination of the drag coefficient for laminar and transition flow using Eq.
(3.10) and Eq. (3.12)
Drag coefficient for laminar flow regime (RH-110)
824
e
DR
C
Drag coefficient for transitional flow regime (RH-70)
53.1)/05.0()/100087.1()3(
)1077.1()/23.998/650,2()/81.94(23
433
smmskg
mmkgmkgsmCD
STEP 3. Calculation of eR
Cd”velocity term” [49] and
2
eDRC “diameter term” [49] value for
transitional flow regime using Eq. (3.13) and Eq. (3.14)
RH-70
17.0)/05.0()/23.998()3(
)/100087.1()/77.1651()/81.94(3
3
smmskg
mskgmskgsm
R
Cd
e
54.117)/100087.1()3(
)1077.1()/23.998()/77.1651()/81.94(3
342
mskg
mmskgmskgsmRC eD
Also, the value of eR
Cd and
2
eDRC can be read from Camp‟s curves (Appendix B).
3)/100087.1(
)/03.0()/23.998()/1004.1(3
34
2
2
mskg
smmkgsmvdR
OH
OHse
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STEP 4. Control calculation of drag coefficient using the yield value of eR
Cd and
2
eDRC
The drag coefficient for transitional flow was determined at Step 2 and gave CD=1.53.
Determination the control value of drag coefficient
From From
53.117.0 D
e
D CR
C 45.154.117
2 DeD CRC
As can be seen from the results, drag coefficient calculated from the “diameter term” was
slightly less than the CD value yield from the general equation of settling velocity (Step 2).
STEP 5. Control calculation of settling velocity using Eq. (3.9)
Settling velocity of 20 individual particles was measured and averaged velocity was
calculated thus, settling velocity of coarse particles was 0.05m/s and fine particles settled
out under 0.03m/s velocity.
Determination of the control value of settling velocity
For RH-70 For RH-110
]/[05.0
3
4
2
2 smC
dgv
OHD
OHss
]/[02.0
3
4
2
2 smC
dgv
OHD
OHss
Control results show that settling velocity of coarse sand was equal with the result obtained
from laboratory analysis. However, control settling velocity of fine sand was 0.01m/s less
than the measured value under laboratory condition. One possible reason of the difference
is human error, the settling velocity was measured in the laboratory using a stop watch.
5.2.2 Determination of Clean-Water Head loss in granular-media filter
During the five phases of filtration experiment, 22 filtered Na-alginate samples were
collected thus, the volumetric flow rates (Q), retention times (t), and filtration rates
(q=vapproach) were calculated. As can be seen from Table 4.2, majority of the fine sand
filtrations were run overnight thus, constant downward flow filtration was not performed.
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As a consequence of this, dual media filter was clogged on 22/07/2009. Filter backwashing
was not operated because the filtration experiment had finished. Head loss through the
filter bed could not be measured because manometer was not installed at the system.
Therefore, the theoretical head loss was determined.
STEP 1. DETERMINATION OF EQUIVALENT HYDRAULIC DIAMETER
It is known, that sphericity is the ratio between the hydraulic diameter (dh) and the
geometric mean of the sieve sizes (ds) Eq. (4.2). Since the sphericity (Table 5.3) and the
average sieves sizes (ds) were known only, the equivalent hydraulic diameter had to be
calculated. Reduced data of sieve analysis and calculation of geometric mean of average
sieves can be found (Appendix I).
TABLE 5.7 ESTIMATED SPHERICITY VALUE AND CALCULATED EQUIVALENT HYDRAULIC DIAMETER
TYPE OF
GRANULAR
MATERIAL
SPHERICITY
(Ψ)
EQUIVALENT
HYDRAULIC
DIAMETER
sh dd [m]
DIAMETER
OF AVERAGE
SIEVES dS [m]
REYNOLDS‟
NUMBER
RH-70
(COARSE)
0.78 1.38x10-4
1.77X10-4
9
RH-110 (FINE) 0.78 8.12x10-5
1.04x10-4
3
Table 5.8, summaries the calculated head loss in a clean filter for small scale, (single
medium systems) and large scale, (single medium systems) using Eq. (3.15). Figure 5.4
(A-F) show volumetric flow rates (Q) versus sampling dates. As can be seen from the
graphs, filtrations were run overnight, thus flow rates were not constant. During Phase I-II.
filtration, fine filter medium (RH-110) purified 25% less Na-alginate solution compare to
RH-70. Downward flow was increased on 18th
June, to establish the most efficient flow
rate for successful filtration of Na-alginate solution. Filter media depth were increased by 5
cm at Phase III. but it had not significantly changed the volume of filtered solution. From
Figure 5.4 F can be seen, overnight operation of the mono media filter had caused 40%
decrease in the volumetric flow rate, which indicates that the filter was being clogged and
filter backwashing would be required.
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TABLE 5.8 VOLUMETRIC FLOW RATES, APPROACH VELOCITIES AND HEADLOSSES DURING
FILTRATION
FILTRATION
TEST
FILTRATION PERIOD VOLUMETRIC
FLOW RATE
(Q) [m3/s]
APPROACH
VELOCITY
vapp=Q/A [m/s]
HEADLOSS IN
CLEAN FILTER
EQ. (3.15) [m]
FILTER MEDIUM
DEPTH
[m] STARTED FINISHED
PHASE I.-II. FILTRATION
SA
MP
LE
CO
DE
RH-70/I. 4.30pm
16th June 09
9am
17th June 09 4.33x10
-9 2.70x10
-5
2.68x10-2
0.25
RH-70/II. 9am
17th June 09
5.15pm
17th June 09
6.17x10-9
3.84x10
-5
3.82x10-2
0.25
RH-70/III. 5.15pm
17th June 09
9.30am
18th June 09 4.67x10
-9 2.91x10
-5
2.89x10-2
0.25
RH-70/IV. 9.30 am
18/06/09
5.15pm
18/06/09 8.00x10
-9 4.98x10
-5
4.95x10-2
0.25
RH-70/V. 5.15pm
18/06/09
12.40 pm
19/06/09 6.17x10
-9 3.84x10
-5
3.82x10-2
0.25
RH-110/I. 4.30pm
16th June 09
9am
17th June 09 3.17x10
-9 1.97x10
-5
6.16x10-2
0.25
RH-110/II. 9am
17th June 09
5.15pm
17th June 09 4.50x10
-9 2.80x10
-5
8.76x10-2
0.25
RH-110/III. 5.15pm
17th June 09
9.30am
18th June 09 4.33x10
-9 2.70x10
-5
8.43x10-2
0.25
RH-110/IV. 9.30 am
18/06/09
5.15pm
18/06/09 7.67x10
-9 4.77x10
-5
1.49x10-1
0.25
RH-110/V. 5.15pm
18/06/09
12.40 pm
19/06/09
4.67x10-9
2.91x10
-5
9.08x10-2
0.25
PHASE III. FILTRATION
SA
MP
LE
CO
DE
RH-70/VI. 4.20pm
30/06/09
9.45am
01/07/09 4.33x10
-9
2.70x10-5
3.50x10-2
0.3
RH-70/VII. 9am
01/07/09
9.30am
02/07/09 6.00x10
-9
3.74x10-5
4.85x10-2
0.3
RH-110/VI. 4.20pm
30/06/09
9.45am
01/07/09 4.33x10
-9
2.70x10-5
3.50x10-2
0.3
RH-110/VII. 9am
01/07/09
9.30am
02/07/09 6.00x10
-9
3.74x10-5
4.85x10-2
0.3
PHASE IV. FILTRATION
SA
MP
LE
CO
DE
DMF-I. 5pm
07/07/09
10am
08/07/09 8.17x10
-9 5.08x10
-5
0.3
DMF-II. 10am
08/07/09
12.40pm
08/07/09
2.40x10-8
1.49x10
-4
0.3
MMF-I. 6pm
07/07/09
10am
08/07/09
8.67x10-9
5.10x10
-6
3.83x10-2
0.6
MMF-II. 10am
08/07/09
12.40pm
08/07/09
5.22x10-8
3.07x10
-5
2.30x10-1
0.6
PHASE V. FILTRATION
SA
MP
LE
CO
DE
DMF-III. 2.30pm
21/07/09
11.20am
22/07/09 7.33x10
-9 4.57x10
-5
0.3
DMF-IV. 11.20am
22/07/09 FILTER BED WAS CLOGGED.
MMF-III. 6pm
21/07/09
10am
22/07/09 1.70x10
-8 1.00x10
-5
1.00x10-1
0.8
MMF-IV. 6pm
22/07/09
9am
23/07/09 9.67x10
-9 5.69x10
-6
5.69x10-2
0.8
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(A) (B)
(C)
(D)
PHASE IV. FILTRATION WAS SHUT DOWN.
(E)
(F)
FIGURE 5.4 (A-F) VOLUMETRIC FLOW RATES VERSUS SAMPLING DATES DURING
PHASE I-III AND V. FILTRATION PERIODS
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5.2.3 Turbidity
During the Phase IV filtration, the effluent became contaminated, consequently,
backwashing was performed and turbidity level was measured. The aim of the
backwashing was to remove the possible material and substances entrapped among the
pores thus, filter bed expansion and backwash flow rates were not measured during the
process operation. However, the theoretical head loss through the filter bed was
determined. Four samples were taken for turbidity analysis after backwashing. As can be
seen from Table 5.9, filter cleaning had been running with Milli-Q water for four days and
the turbidity level significantly decreased from the initial concentration of 102.5 NTU to
2.4 NTU. Comparing the final sample concentration to the control sample (Milli-Q water),
it can be clearly seen that the effluent was still turbid but due to lack of time for the
experiment the filter cleaning step was stopped. Therefore, there is a possibility that
filtered Na-alginate solutions physical properties were modified due to the contamination.
TABLE 5.9 TURBIDITY LEVEL AND CONCENTRATION (NTU) OF THE EFFLUENT SAMPLES AFTER
BACKWASHING
EFFLUENT SAMPLES
(AFTER BACKWASHING)
TURBIDITY
(NEPHELOMETRIC
TURBIDITY UNITS=NTU)
TURBIDITY
CONCENTRATION
(%)
16/07/2009 102.5 34,067%
17/07/2009 88.8 29,500%
20/07/2009 4.59 1,430%
21/07/2009 2.4 700%
Milli-Q water (Control
sample)
0.3 0
5.2.3.1 Calculation of the theoretical head loss in fluidised
Porosity
nRH-110=0.422
32650
m
kgS
Filter bed depth before backwashing
L=0.8m )20(2 CTOH
=998.23
3m
kg
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mLnhOH
OHS 77.0)(
12
2
(5.1)
5.3 Evaluation of the viscosity measurements of sodium alginate solutions
The goals of the analysis were to determine the rheological properties of aqueous Na-
alginate under conventional and extreme conditions, and to evaluate the effects of the
filtration method on the solution viscosity. It is well known that molecular weight,
temperature and solution concentration affect the viscosity, which determines the size and
shape of the alginate beads. Table 5.10 summarises the prepared samples for the analysis.
Viscosity of the samples was measured at 25°C unless otherwise stated.
TABLE 5.10 PREPARED SAMPLES FOR VISCOSITY ANALYSIS
SAMPLE CODES SOLUTION CONCENTRATION
(%)
COMMENTS
CONTROL SAMPLES 0.25%, 0.5% 1%, 1.25%,
1.5%, 1.875%, 2%, 2.5%, 3%,
3.5%, 4%
Fresh NaAlg solution and
autoclaved *
FRESH ALGINATE 0.2%, 2% autoclaved
not lyophilised
2% was measured at 25°C
and 37°C
0.2%, 2% not autoclaved
not lyophilised
0.2%, 2% autoclaved
not lyophilised
UNFILTERED
NaAlg SOLUTION
0.2%, 2% autoclaved
lyophilised
OLD NAALG SOLUTION 0.2%, 2% 1 week old sample
RH-70 0.2%, 2%
autoclaved
lyophilised RH-110
DMF 0.2%, 2%
autoclaved
lyophilised MMF
(*) Sterilisation of the sample at 121°C for 10mins unless otherwise stated.
The results of the analysis were plotted on three different graphs i.e. dynamic viscosity as a
function of shear rate and shear stress, and the flow curves, which shows the Newtonian or
non-Newtonian behaviour of the fluids. Viscosity of a Newtonian fluid changing by stress
and temperature but independent of shear rate, whereas a non-Newtonian fluid viscosity
highly dependent on these three factors.
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In the following sections, the flow curves are presented and the majority of the analysis can
be found (Appendix J).
5.3.1 Effect of different concentration on solution viscosity
Figure 5.5 A-D shows the shear stress as a function of shear rate (flow curve) of various
alginate solution concentrations.
(A)
(B)
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(C)
(D)
FIGURE 5.5 A-D FLOW CURVES OF NEWTONIAN AND TIME-INDEPENDENT NON-NEWTONIAN
FLUIDS. FLOW CURVES SHOW THE RELATIONSHIP BETWEEN SHEAR STRESS (Pa) AND SHEAR
RATE (1/S) FOR VARIOUS ALGINATE CONCENTRATIONS.
As can be seen from Figure 5 (A), flow curves of 0.2% and 0.25% NaAlg solutions are
linear confirming these samples as exhibiting Newtonian fluid behaviour. As a result, the
assumption was made in Section 3.5.5 was verified. Figure 5 (B-D) show, the fluids
behaviour was changed by increasing the solutions concentration. As a result of this, the
assumption that alginate solutions below 0.5% shows Newtonian characteristic made in
Section 3.5.5 was verified.
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Figure 5 B-D show, the fluids behaviour was changed by increasing the solutions
concentration. As a result, the viscosity of the solutions was gradually decreasing as shear
rates were increasing. These systems showed non-Newtonian (pseudoplastic) fluid
properties.
5.3.2 Effect of autoclaving on solution viscosity
Table 5.11 shows the effect of autoclaving on the 0.2% and 2% aqueous Na-alginate
solutions viscosity, measurement were made at 25°C. The effects of the sterilisation can be
seen on Figure 5.6-5.7. A 82% decrease in the viscosity of 2% NaAlg solution autoclaved
for 20mins was measured compared to a reduction of 40% for 2% alginate autoclaved for
10mins. Clearly it can be seen from Table 5.11 and Figure 5.6-5.7, that 20mins autoclaving
caused higher degree of depolymerisation of the uronic acid residues. Flow curve of a 2%
NaAlg solution after 20mins heat treatment almost showed Newtonian fluid characteristic.
Autoclaving altered the physical characteristic of the alginate solution therefore, the size
and sphericity of the beads could be affected which may result a decline in cell growth and
viability.
TABLE 5.11 EFFECT OF AUTOCLAVING AT 121°C FOR 10 AND 20MINS ON THE VISCOSITY OF NAALG
SOLUTIONS
NA-ALGIANTE
CONCENTRATION (%)
VISCOSITY OF THE SOLUTIONS (Pa s)
NON-AUTOCLAVED AUTOCLAVED
(10MINS)
AUTOCLAVED
(20MINS)
0.2 0.007 0.07
0.25 0.008
2 0.802 0.480 0.143
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FIGURE 5.6 DYNAMIC VISCOSITY OF 0.2% NAALG SOLUTION AS A FUNCTION OF
SHEAR STRESS (Pa)
FIGURE 5.7 FLOW CURVES OF AUTOCLAVED NaAlg (CONTROL) SOLUTIONS
5.3.3 Effect of temperature on solution viscosity
The effects of temperature on the alginate solution show in Figure 5.8. The viscosity of the
solution decreased by almost 34% at 37°C compared to the viscosity at 25°C. Flow curves
demonstrated (Figure 5.9) that non-Newtonian behaviour of the fluid significantly
decreased by increased temperature. Moreover, a 2% NaAlg solution at 37°C showed
almost Newtonian behaviour. The temperature results demonstrated the sensitivity of
alginate to increased heat.
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FIGURE 5.8 VISCOSITY OF 2% NAALG SOLUTION AT DIFFERENT TEMPERATURES
FIGURE 5.9 FLOW CURVES OF 2% NAALG SOLUTION AT DIFFERENT TEMPERATURES
5.3.4 Effect of filtration on the solution viscosity
Figure 5.10-5.11 represent the viscosity changes of 0.2% alginate solutions compared to
non-filtered aqueous Na-alginate after fine and coarse sand, mono medium and dual media
filtration. It can be seen from Figure 5.10 that non-filtered but freeze-dried, and autoclaved
0.2% sample was pseudoplastic compared to the purified sodium alginate solutions, which
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exhibited Newtonian fluid characteristic. Clearly, viscosity of a pseudoplastic fluid
changes by increased shear rate, whereas viscosity of a Newtonian fluid is staying
constants by increasing shear rate. Viscosity has the greatest effect on alginate gel
properties and due to the dilution and filtration process alginate solutions lost its strength
and caused non-spherical beads morphology during encapsulation. This could be one of the
reasons for the cells viability and growth decline.
FIGURE 5.10 FLOW CURVES OF FINE SAND FILTERED 0.2% NA-ALGINATE SOLUTIONS
FIGURE 5.11 FLOW CURVES OF MONO MEDIUM AND DUAL MEDIA FILTERED 0.2% NA-ALGINATE
SOLUTIONS
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5.4 Reconstruction of sodium-alginate
5.4.1 Evaluation of the effect of fine sand filtration on the size distribution of the
particulates
Figure 5.12 indicates, the broad spectrum of micron particulates presented in non-purified
2% sodium alginate solution. During the filtration period, the particulate size was lowered
in the solution compared to non-purified sample and Figure 5.13 A-B and Figure 5.14 A-B
show the effect of coarse and fine sand filtration on the particulate length distribution of
filtered Na-alginate. As can be seen from the graphs, fine sand filter removed larger micron
particulates compared to coarse sand. Increasing downward flow had slightly changed the
removal efficiency of the filtered thus, less micron particles were removed. Particles size
and shape has significant effect on the filtration efficiency therefore, it was difficult to
design an effective filtration system because the size distribution of particulates in alginate
suspension was not known. It is also important to know the surface characteristics such as
surface charge of the particles, which is predominant for micron size particles, in the
surrounding fluid [65].
During filtration suspended particles interacts with the liquid causing repulsion or
attraction. These factors would determine the settling behaviour of the particulates. If
particle size distribution of aqueous Na-alginate had known, a more effective filter media
system would have designed.
FIGURE 5.12 PARTICLE SIZE DISTRIBUTION OF NON-PURIFIED 2% SODIUM ALGINATE SOLUTION
MEAN PARTICLE SIZE
5µM±2µM
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(A)
(B)
FIGURE 5.13 LENGTH DISTRIBUTION (µm) OF PARTICLES IN RH-70 SAND FILTERED NAALG
SOLUTION. (A) PARTICLES LENGTH UNDER SLOW FLOW RATE (B) PARTICLES LENGTH UNDER
INCREASED FLOW RATE
RH-70 (coarse sand),
increased flow rate
MEAN PARTICLE SIZE
4.70µm
RH-70 (coarse sand), slow
flow rate
MEAN PARTICLE SIZE
4.43µm
PARTICLE SIZE (µm)
PARTICLE SIZE (µm)
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(A)
(B)
FIGURE 5.14 LENGTH DISTRIBUTION (µm) OF PARTICLES IN RH-110 SAND FILTERED NAALG
SOLUTION. (A) PARTICLES LENGTH UNDER SLOW FLOW RATE (B) PARTICLES LENGTH UNDER
INCREASED FLOW RATE
RH-110/III. (fine sand),
slow flow rate
MEAN PARTICLE SIZE
3.60µm
RH-110/I. (fine sand),
increased flow rate
MEAN PARTICLE SIZE
3.90µm
PARTICLE SIZE (µm)
PARTICLE SIZE (µm)
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Figure 5.15 show the removal efficiency of Phase V filtration. Although sand depth was
0.80 m, particulates reduction had not changed significantly compared to small scale
filtration run. Large scale filtration system was operated less efficient due to the
contaminated filter medium. Although filter backwashing was performed, the turbidity
level of the effluent was not decreased to 0.3NTU. The smaller particulates could not
percolate through the filter bed because of the entrapped organic and probably inorganic
impurities in the filter medium.
FIGURE 5.15 PARTICLES LENGTH DISTRIBUTION (µm) OF LARGE SCALE FINE SAND FILTERED
NAALG SOLUTION
After Phase I-III filtration experiment, firstly, it could be determined that fine sand filter
retained larger micron particulates compared to coarse sand. Secondly, slow downward
flow rate was more efficient compared to increased flow. Therefore, the filter media were
operated at slow downward flow rate during Phase IV-V filtration.
PARTICLE SIZE (µm)
MMF-II. Large scale, fine
sand filtration.
Sand depth 0.8m
MEAN PARTICLE SIZE
3.97µm
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5.4.2 Evaluation of particle size measurement of filtered sodium alginate solutions
Particle size measurements of filtered Na-alginate solutions were carried out at
Hepatology, Royal Free Hospital. Results obtained from the analysis were used to calculate
the particles size and number distribution of 1g Na-alginate powder, which can be seen
from Figure 5.16. Detailed calculation of particle size measurement can be found
Appendix K.
FIGURE 5.16 DISTRIBUTION OF PARTICLES SIZES (µm) AND NUMBERS OF NA-ALGINATE
POWDER
As can be seen from the results, the most contaminated sample was the unpurified and non-
autoclaved Na-alginate solution. During the filter run almost all large (10-20µm)
particulates were removed from the solutions. An 82% decrease in the number of 2µm
particulates of autoclaved solution was detected compared to raw Na-alginate solution.
Dual media filter had eliminated 5-10µm particulates and 94% of 2µm particulates
compared to unfiltered alginate solution. Mono medium filter (MMF) and fine sand filter
removal efficiency of 2µm were almost the same. The reason of the inadequate MMF
operation compared to small scale RH-110 filter was the contaminated filter bed.
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5.4.3 Encapsulation of filtered sodium-alginate
As a consequence of the fine sand filtration experiment, viscosity of the sodium alginate
solution was changed. Since the aim of the encapsulation was to produce micron beads
with spherical shape, the Na-alginate concentrations -1.25%, 1.5%, 1.75%, 1.87%, and 2%
- were analysed and compared to 1.0% normally used.
5.4.3.1 Empty beads morphology
As can be seen from Figure 5.17 beads formed from non-purified Na-alginate solution had
more spherical geometry compared to microcapsules prepared from purified alginate
Figure 5.18. At the first encapsulation stage a 2% alginate solution was used for empty
microcapsulation. Stretch marks Figure 5.18 were found on the surface of the microbeads,
moreover the shape of the beads were non-spherical. Additional to this, decreasing the
solution concentration caused more deformed, non-spherical beads and irregular sizes.
As can be seen, the solution properties of alginate strongly dependent on the viscosity,
which could be affected by the molecular weight of the polymer, concentration and
possible residual impurities. Sodium alginate powder was research grade, thus information
regarding the chemical composition of the polymer was not available.
As the encapsulation process went further, it was found that, 1.875 % purified alginate
solution gave more homogeneous beads, which is another important parameter of alginate
beads in application for immobilising living cells. Therefore, HepG2 cells were
encapsulated in 1.875% DMF and MMF filtered solutions.
FIGURE 5.17 ALGINATE BEADS FROM NON-PURIFIED 2% SODIUM ALGINATE SOLUTION
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A C
B D
FIGURE 5.18. EFFECT OF THE NA-ALGINATE SOLUTION CONCENTRATION ON THE MORPHOLOGY
AND SIZE OF EMPTY ALGINATE BEADS. BEADS WERE PREPARED USING 1.25% (A) AND 1.5% (B)
DMF FILTERED SOLUTION; C 1.75% MMF FILTERED SOLUTION AND D 2% FINE SAND FILTERED
AQUEOUS NA-ALGINATE.
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5.5 Encapsulation of HepG2 cells
5.5.1 Morphology of cell cultured alginate beads
Alginate micro spheres from mono medium filtered sodium alginate were more spherical
(Figure 5.19) than beads from dual media filtered alginate at day 4 (Figure 5.20).
FIGURE 5.19 PHASE 4: ENCAPSULATED HEPG2 CELLS; MONO MEDIUM FILTERED 1.875% SODIUM
ALGINATE SOLUTION WAS USED FOR CELL IMMOBILISATION
FIGURE 5.20 PHASE 4: ENCAPSULATED HEPG2 CELLS; DUAL MEDIA FILTERED 1.875% SODIUM
ALGINATE SOLUTION WAS USED FOR CELL IMMOBILISATION
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5.5.2 Protein production from encapsulated HepG2 cell
Curves are showing the protein synthesis as a function of time for three different purified
alginate culture conditions (Figure 5.24). As can be seen, protein production from dual
media filtered (DMF) alginate encapsulated HepG2 cells were lower than mono media
filtered at day 9 of culture. The largest production in albumin was at day 9 for mono media
filtered and non filtered alginate entrapped HepG2.
FIGURE 5.24 ALBUMIN (PROTEIN) PRODUCTION FROM ENCAPSULATED HEPG2 CELLS IN A NON
FILTERED, MONO MEDIUM, AND DUAL MEDIA FILTERED ALGINATE SOLUTION
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5.5.3 Assessment of cell viability in alginate beads
Figure 5.21 shows the viability of the purified sodium alginate encapsulated HepG2 cells
compared to non filtered microcapsules. As can be seen from the graphs, at day 5 viability
of the cells reached a peak. HepG2 cells cultured in non filtered and mono media filtered
alginate beads had levelled out between days 5-15 compared to cells maintained in the non
filtered alginate matrix; viability of the cells were significantly lower. It is unclear what
caused this decrease, it may have been due to the lack of support provided by the beads, or
potentially an anomalous result. The experiment would need to be repeated to confirm this.
FIGURE 5.21 VIABILITY OF ENCAPSULATED HEPG2 CELLS IN A NON FILTERED AND MONO MEDIUM,
AND DUAL MEDIA FILTERED ALGINATE SOLUTION
Figure 5.22 demonstrates that cells number of mono media purified alginate encapsulated
HepG2 cells slightly declined compared to cells in non purified alginate beads. It also can
be seen, that the dual media filtered alginate solution had the greatest impact on alginate
solution properties, cells number dropped below 2x10-6
.
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FIGURE 5.22 CELLS NUMBER OF PURIFIED AND NON PURIFIED ALGINATE ENCAPSULATED HEPG2
CELLS
Analysis of FDA and PI stained beads using confocal microscopy showed a low number of
dead cells in both mono media filtered and dual media filtered at day 4 (Figure 5.23).
Overall, there is a clear difference between HepG2 cells encapsulated in non filtered
alginate, DMF and MMF.
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(A) DAY 3 LIVE HEPG2 CELLS; DMF (C)DAY 3 LIVE HEPG2 CELLS; MMF
(B) DAY 3 DIED HEPG2 CELLS; DMF (D) DAY 3 DIED HEPG2 CELLS; MMF
FIGURE 5.23 LIVE AND DEAD ENCAPSULATED HepG2 CELLS IN MONO MEDIUM AND DUAL MEDIA
FILTERED ALGINATE MICROCAPSULES AT DAY 3 STAINED WITH FDA AND PI.
(A) DMF FILTERED NaAlg ENCAPSULATED CELLS GROWTH AND (B) CELLS DECLINE.
(C) MMF FILTERED NaAlg ENCAPSULATED CELLS GROWTH AND (D) CELLS DECLINE.
GREEN SHOWS LIVE CELLS, AND READ REPRESENT DEAD CELLS.
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6 CONCLUSIONS
The hypothesis of the dissertation was that sand filtration would remove micron particulates
from aqueous sodium alginate, thereby providing a biocompatible polymer matrix for cell
encapsulation. It was believed that sand filtration could act as a promising purification process
for large scale production of purified alginate without altering the physical composition of the
polymer. Therefore, the micron particulates removal efficiency of the sand filtration was
investigated by setting up various filtration systems. As was described in this dissertation, it
was revealed that filtering sodium alginate solution through a dual media filter could
eliminate micron particulates between 10 to 20µm, and reduced 94% of 2µm particulates
compared to non filtered Na-alginate solution. Filtration process showed a major impact on
the dynamic viscosity of the solution, even thought the micron particulates were removed to
some extent. As a consequence of this, the stability and the morphology of the micro beads
were hugely affected. Furthermore, it was showed that immobilisation of HepG2 cells in fine
sand filtered, aqueous sodium alginate had not provide a coherent gel matrix for the cells.
The following findings and conclusions of this work had contributed to understand the
disadvantages of solid-liquid based purification of sodium alginate, therefore providing an
idea for a unique and an alternative purification method, which is presented in the
recommendation chapter.
The results of the sand filtration experiment have shown that during the first stage of the
investigation; fine sand (RH-110) filter had greater removal efficiency for particulates
between 2µm and 5µm compared to coarse sand (RH-70) and to the particulate size
distribution of non filtered sodium alginate solution. Mean particle size removal of fine sand
was 3.60µm whereas coarse sand 4.43µm under slow flow rate. Varying the flow rate during
Phase I-II filtrations had resulted to purify more sodium alginate but there was a decline in the
particulates removal efficiency. Fine sand filter could purify 0.39ml more alginate solution for
the fourth sampling compared to the first sample. For the same period, coarse sand filter
purified 0.32ml more than at the first sampling.
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Increasing, the inflow rate gave higher volumetric flow rate but provided less purified alginate
solution. Moreover, filtration time (t) was between 0.73 and 1.02 days for fine and coarse
sand filter. The results indicated that the filter was being clogged and the headloss was
increased. It is necessary to mentioned, Phase I-III filtration experiments were small scale
systems, filters were running overnight and that problem was accumulated more during Phase
V filtration when dual media filter become clogged.
This work has also showed that filter bed was contaminated due to insufficient cleaning
process, which was described in section 4.4. During Phase IV-V the filter media was not clean
before filtration; therefore it could not provide acceptable purity level for sodium alginate
solution. Although the turbidity level of the mono media filtered effluent was reduced to
2.4NTU from the initial 102.5NTU concentration, the filter was not purely clean. This
probably increased the impurity content of the filtered Na-alginate solution.
What has been revealed from the viscosity measurement enabled to understand the
rheological properties of the polymer solution and the analysis showed the complexity of the
aqueous sodium alginate. At the concentration spectrum of 1% to 4% the viscosity behaviour
of alginate solution was pseudoplastic. Any decrease in concentration altered the dynamic
viscosity of the solution, thus providing a thin fluid like water and it determined the effect on
the cell encapsulation. Several encapsulation tests were undertaken to identify the most
suitable concentration for spherical alginate beads production. As a consequence of this, it
was shown that 1.875% filtered sodium alginate solution gave more spherical beads but the
size distribution of the beads were multiform.
The work had highlighted that viscosity of sodium alginate decreased by not only
concentration, temperature, time but also autoclaving. Increasing temperature by 12°C a 2%
alginate solution showed almost Newtonian fluid characteristic. This finding suggests that
increasing temperature even higher would lead to a total loss in thickness of the fluid.
Autoclaving a 2% alginate solution for 20mins had drastically decreased the dynamic
viscosity of the fluid compared to a non autoclaved sample; viscosity dropped by 82%.
The solution property of alginates not only depends on the viscosity but also on the chemical
composition and impurities presented in the powder of sodium alginate. The study has
reinforced the impact of unknown detailed chemical and composition analysis of the polymer
since, it made difficult to be able to better predict the reasonable outcome of the filtrations.
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This research has also shown that immobilisation of HepG2 cells within mono medium and
dual media filtered (DMF) alginate spheres had altered the growth of cells, although function
as measured by albumin was relatively unaffected compared to cell number and protein
synthesis of the cells compared to unfiltered spheroid cultures.
Growth function of HepG2 cells cultured in DMF had dropped below 2x10-6
between days 4
and 9 and gradually started to increase, and at day 14 had reached its peak (10x10-6
). Same
process was observed during viability, when after a sudden increase at day 9 the viability of
the cells dropped by 2%. Albumin (protein) production of DMF HepG2 microspheres was
flocculating. Protein content of cell at day 4 and 12 was on peak, reaching 7µg/million. Mono
media filtered (MMF) micro bead had least modified the growth, function, and viability of the
cells compared to DMF. Viability of HepG2 cells entrapped in the flexible matrix was
levelled out between day 5 and 10. Albumin production of the cells had fall to 6µg/million by
day 6 compared to 8µg/million of unfiltered beads by the same time.
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7 RECOMMENDATIONS
The experimental works were evaluated not only by engineering and medical science aspects
but also the efficiency of the currently publish purification processes were put into
consideration [14, 18-19, 25]. Therefore, a key question was addressed:
“Is the liquid-solid based purification method the most appropriate for the purification of
“micron particulates free” alginate biopolymer suitable for cell encapsulation?”
For immobilisation of cells in alginate matrix, the most important property is the polymer‟s
viscosity. As could be seen, many published in-house purification protocols and the fine sand
filtration had utilised alginate solubility in water. Thus, liquid-solid separation processes have
been investigated for alginate purification.
In this section, an alternative approach for alginate purification, utilising dry alginate powder
in a cyclonic separation from gas stream and possible production of “micron particulate free”
alginate for cell encapsulation is discussed. Utilisation of cyclones are diverse in various
science and engineering technologies, for instance air pollution control, spraying of
pharmaceutical drugs, and powders classification on the basis of their physical and chemical
properties [66-67]. It is important to mention, that the proposed separation process would be a
unique solution for alginate purification and it might help to optimize the rheological
behaviour of the polymer.
As can be seen from, Figure 7.1 micron and macro particles (2µm-1000µm) can be removed
from gas streams by cyclones.
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TIMEA GREGO 85
FIGURE 7.1 PARTICLE SIZE DISTRIBUTION OF SEVERAL MATERIALS ( ) IN A FUNCTION OF
SEPARATION TECHNIQUES ( ); CYCLONES SEPARATION PARTICLE SIZE 1µm-1,000µm [66].
7.1 Operation of the gas-solid cyclone
The operation of the commonly designed cyclone is based on reverse flow where particles are
suspended in a gas stream and separated by centrifugal force [66]. Figure 7.2 shows a
schematic diagram and process steps of a reverse flow cyclone.
FIGURE 2 REVERSE FLOW CYCLONE SEPARATOR. SUSPENDED PARTICLES IN GAS ENTER IN THE CYCLONE AND
CENTRIFUGAL FORCES (VORTEX) DRIVE THEM TO THE CENTRAL PART, WHERE THE PARTICLES WILL BE SEPARATED
[68.]
Separation processes
Particles size range of
different materials
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TIMEA GREGO 86
Cyclones can be categorised by their size such as large- and small cyclones, which is more
efficient in particulates removal below 5µm [70]. Figure 7.3 shows the grade efficiency curve
of cyclones separator. As can be seen from the diagram, 50% of micron particles (~6µm) can
be removed from gases by cyclones.
FIGURE 7.3 GRADE EFFICIENCY CURVES OF GAS-SOLID SEPARATION DEVICES VERSUS PARTICLE SIZE (µm)
CYCLONES REMOVE 50% OF THE PARTICLES (6µm) [68]
Successful design and separation efficiency of micron particulates from gases depends on the
following factors [66]
1. Physical factors of the powder
Particle size: it is suggested to undertake a detailed particle size distribution
analysis of the polymer powder because it will determine the behaviour of the
particles under certain conditions. Analysis would involve a “direct-, indirect-
and a classification methods” [69]. Direct technique will estimate the size of
individual alginate particles, whereas indirect system will determine the
chemical characteristic of the particles. It is important to mention, there has not
been established a polymer texture classification standard for alginate powder.
Particle Shape has the greatest impact on the separation efficiency.
Density
2. Chemical composition of the powder
Determination of molecular weight (Mw): Mw has an influence on the viscosity
of alginate solution. Mw can be determined by measuring the intrinsic viscosity of the
polymer solution [71].
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TIMEA GREGO 87
To summarise, the solid-gas purification process presented might be used as an alternative
purification method for micron particulates removal of alginate, and for the production of
large scale purified alginate for clinical use. The system utilises gas thus there is a possibility
that physical composition of Na-alginate will not be altered significantly. However, further
study needs to be undertaken to validate the above stated therefore, the following process
stages are suggested
Stage 1. Detailed physical and chemical characterisation of Na-alginate and a feasibility study
of the proposed purification method,
Stage 2. System Design in accordance with Stage 1,
Stage 3. A laboratory scale System Architecture based on Stage 1-2,
Stage 4. Cyclone separation of suspended Na-alginate powder in gas and particulates removal
between 1-6µm,
Stage 5. Sterilisation of purified alginate before cell encapsulation,
Stage 6. Preparation of purified Na-alginate solution for cells encapsulation and viscosity
measurement,
Stage 7. Viability analysis of HepG2 cells.
The length of the dissertation is: 15,885 words
(exc. of references, table of contents, index, acknowledgements and appendices)
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31. Dumitriu, S. Polymeric biomaterials ISBN -0-8247-0569-6
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34. Hoek C., Mann D. G., and Jahns H. M. Algae: An introduction to phycology.
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43. Picture of Darcy‟s Law
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48. Reyolds, T. D. and and Richards, P. A. „Unit Operations and Processes in
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58. Standard Operating Procedure for making 2% HEPES buffered alginate solutions.
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61. Franks, F. „Freeze-drying of Pharmaceuticals and Biopharmaceuticals‟.
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68. Rhodes, M. (2008) „Introduction to Particle Technology‟. John Wiley&Sons.
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APPENDICES
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A. RECENTLY PUBLISHED IN HOUSE PURIFICATION METHODS
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ALGINATE PURIFICATION METHODS
METHODS AUTHOR AND YEAR OF
PUBLICATION
REMOVED IMPURITIES ADVANTAGES DISADVANTAGES
ENDOTOXIN MITOGENIC
IMPURITIES
POLYPHENOL PROTEINS
CHEMICAL PURIFICATIONS
1. FREE FLOW
ELECTROPHORESIS
(FEE) [10]
(SEE FIGURE 3.7.)
Zimmermann U. et al.
(1992)
+ + D/M D/M
- Endotoxin level was
almost zero after
purification
- Alginates with
different ration of
mannuronic acid and
guluronic acid can be
treated
- Expensive
equipments are
required,
- Extremely long process,
- Not suitable for large
scale purified alginate
production.
- Viscosity of the
purified alginate was
changed
- Fibrotic overgrowth
around micro beads
2. ‘MULTI – STEP’
PURIFICATION
PROCESS [9]
Vos, P., De Haan, B.
J., Wolters, G. H. J.,
Strubbe, J. H., Van
Schilfgaarde, R.
(1997)
„Improved
biocompatibility but
+ D/M + +
- Before and after the
purification process,
there was no
mannuronic- and
guluronic acid content
changes observed
- Improved the
- Alginate beads had
fibrotic overgrowth
between 10-30%
- Limited graft function
as a consequence of
fibrotic tissues.
- Proteins content did
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limited graft survival
after purification of
alginate for
microencapsulation of
pancreatic islets‟
Diabetologia (1997)
40: 262-270
biocompatibility of
alginate beads as a
result of endotoxin and
protein level reduction.
- Endotoxin content
was drastically lower
than in the non-
purified alginate. [3]
- Polyphenols content
was much lower
compare to the non-
purified alginate. [3]
not changed
significantly in two
purified alginates
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METHODS AUTHOR AND YEAR OF
PUBLICATION
REMOVED IMPURITIES ADVANTAGES DISADVANTAGES
ENDOTOXIN
(PYROGENS)
[7]
MITOGENIC
IMPURITIES
POLYPHENOL PROTEINS
CHEMICAL PURIFICATIONS
3. SIMPLIFIED
‘MULTI – STEP’
PURIFICATION
PROCESS [7]
Prokop, A. and Wang,
T. G. „Purification of
polymers used for
fabrication of an
Immunoisolation
Barrier‟ Annals New
York Academy of
Sciences
+ + + [3] + [3]
- Endotoxin removal
by charcoal
- after purification,
the endotoxin levels
were still too high
(ASTM [1] guide stated
endotoxin level should
be below 5 EU/kg of
body weight)
4. THREE PHASE
PARTITIONING
METHOD (TPP)
Sharma, A. and Gupta,
M. N. „Three phase
partitioning of
carbonhydrate polymers:
separation and
purification of alginates‟
(2001)
D/M D/M D/M +
- „Elegant technique‟
[15] for elimination of
protein content of
alginate
- „easily scalable‟
[15]
- The test was carried
out on 2 ml alginate
solutions
- There was no
information regarding
the chemical components
of the alginate
- The viscosity of the
non-Newtonian polymer
was not measured. It is
understandable because
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Symbols: (+) can be removed; (-) not suitable method for removal; (D/M) does not mention
of the prepared amount
of alginate.
- Further research is
needed whether this
method is suitable for
large scale alginate
purification.
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B. CAMP’S CURVES OF
2
ed
e
d RandCR
C
VERSUS RE
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C. CHEMICAL ANALYSIS OF RH-70 AND RH-110
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D. GRAIN SIZE DISTRIBUTION ANALYSIS OF RH-70 AND RH-110
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E. TECHNICAL DRAWING OF LARGE SCALE SYSTEM
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F. SPHERICITY AND ANGULARITY GRAPHS
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G. SETTLING VELOCITY OF INDIVIDUAL SAND GRAINS
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H. DETAILED CALCULATION OF HYDRAULIC OF FILTRATION
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I. REDUCED DATA FROM SIEVE ANALYSIS
AND BS 410:1986
SPECIFICATION FOR TEST SIEVES [52]
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MESH NUMBERS
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MESH
NUMBERS
INTERVAL
OF MESH
NUMBERS
BS STANDARD
SIEVE NOMINAL
APERTURES (µm)
[52]
BS
SIEVE
SIZE
[mm]
AVERAGE SIEVE SIZE
(dS)
RH-70 RH-110
22 22-30
710 0.710 0.60
25 600 0.600
30 30-44
500 0.50 0.43
36 425 0.425
44 44-60
355 0.355 0.30
52 300 0.300
60 60-85
250 0.25 0.21 0.21
72 212 0.212
85 85-120
180 0.18 0.15 0.15
100 150 0.15
120 120-170
125 0.125 0.11 0.11
150 106 0.106
170 170-240
90 0.090 0.08 0.08
200 75 0.075
240
240-440
63 0.063
0.05 0.05
300
<63
53 0.053
350 45 0.045
400 38 0.038
440 32 0.032
Geometric mean of average sieve size 0.177 0.04
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J. RESULTS OF THE VISCOSITY ANALYSIS
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K. PARTICLE SIZE MEASUREMENT OF
FILTERED SODIUM ALGINATE SOLUTION