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TITLE
DEVELOPMENT OF A FLICKING SYSTEM FOR PRODUCING 3-DIMENSIONAL
CELLS IN MICROBEADS
WONG SOON CHUAN
A thesis submitted in
fulfilment of the requirement for the award of the
Degree of Master in Electrical Engineering
Faculty of Electrical and Electronic Engineering
Universiti Tun Hussein Onn Malaysia
OCTOBER 2016
iii
DEDICATION
For my beloved family
iv
ACKNOWLEDGEMENT
Thanks to God for all the blessings given to me, both in wisdom and health that I am
able to finish this project successfully. Special thanks to my supervisor, Assoc. Prof. Dr.
Soon Chin Fhong for her supports, patience and guidance given throughout the duration
for this research. We acknowledge the help from Prof. Dr. Cheong Sok Ching from
Cancer Research Malaysia for donating oral squamous cell carcinoma (ORL-48) cells to
this research. Continuous research discussion and supports from the colleagues from
Biosensor and Bioelectronics Laboratory, MiNT-SRC and FKMP, UTHM is another
important factor that helps in the completion of this project. Appreciation is also
extended to the lecturers or panels from FKEE who has provided constructive criticism
in improving the research.
Not forgetting all my friends whom always being there for me when I needed
them most. Appreciation also goes to everyone involved directly and indirectly towards
the compilation of this thesis. Thanks also to my family members for giving me the all
the support that I need in completing this project and thesis especially in spiritual and
financial support.
v
LIST OF ASSOCIATED PUBLICATION
Journal
1. Soon Chuan Wong, Chin Fhong Soon, Wai Yean Leong, Kian Sek Tee,
“Flicking technique for microencapsulation of cells in calcium alginate leading
to the microtissue formation”, Journal of Microencapsulation, Volume 33, Issue
2, Pages: 162-171, 11 February 2016. http://dx.doi.org/10.3109/02652048.2016.
1142017. Impact factor: 1.631 (Q2, JCR, ISI Indexed).
2. Soon Chuan Wong, Chin Fhong Soon, Wai Yean Leong, Kian Sek Tee,
“Development of a flicking system for producing calcium alginate microbeads”,
Jurnal Teknologi, Volume 78, Issue 6-2, Pages: 103-109, June 2016.
http://dx.doi.org/10.11113/jt.v78.8909 (Scopus Indexed).
3. Wai Yean Leong, Chin Fhong Soon, Soon Chuan Wong, Kian Sek Tee,
“Development of an electronic aerosol system for generating microcapsules”,
Jurnal Teknologi, Volume 78, Issue 5-7, Pages: 79-85, May 2016.
http://dx.doi.org/10.11113/jt.v78.8718 (Scopus Indexed).
vi
Conference proceeding
1. Chin Fhong Soon, Soon Chuan Wong, Wai Yean Leong, Mohd Khairul Ahmad,
Kian Sek Tee, “A flicking method for generation of polymer microbeads”,
Japanese Journal of Applied Physics (JJAP) Conference Proceedings, Volume 4,
011110 (2016) doi:10.7567/JJAPCP.4.011110, 14th
International Conference on
Global Research and Education, Inter-Academia 2015, September 28-30, 2015,
Hamamatsu, Japan.
vii
LIST OF AWARD
1. Gold Medal in Research & Innovation Festival 2015 (UTHM),
“A novel flicking system for producing high throughput 3D cells”,
16 – 17th
November 2015, Universiti Tun Hussein Onn Malaysia.
2. Bronze Medal in Malaysia Technology Expo (MTE) 2016,
“A novel flicking system for producing high throughput 3D cells”,
18 – 20th
February 2016, Putra World Trade Centre, Kuala Lumpur, Malaysia.
PATENT FILING
1. In the process of patent filing. (Patent pending)
“Novel flicking system for producing high throughput 3D cells”
viii
ABSTRACT
Culturing cells on planar compliant substrates produces low yield of microtissues. A
variety of microtechnologies was introduced and developed to encapsulate cells for
producing microtissues. However, the size control of the microcapsules is challenging to
the current technologies for cells encapsulation. In this research, we proposed a simple
yet efficient technique to encapsulate cells leading to the growth of microtissues. The
technique involved with the development of a flicking system which can be applied to
encapsulate cells in calcium alginate microbeads at different flow rates and flicking
speed. The microbeads size increased with the flow rate but decreased with the flicking
speed. Flicking speed of 80 rpm and flow rate of 4 µl/min was chosen to use in the cells
encapsulation. The cells encapsulated in the microbeads at cell density of 31.9 × 106
cells/ml (HaCaT) and 94.2 × 106 cells/ml (ORL-48) were cultured and observed for
proliferation over a period of time. The microbeads had a smooth surface with spongy
and porous surface texture in FE-SEM imaging. In nucleus (DAPI) staining, the
encapsulated HaCaT and ORL-48 cells in microbeads grew from scatter individual cells
to form cells aggregate and then microtissues. In live and dead cells stainings, majority
(≈99 %) of the microtissues cultured in the calcium alginate microbeads were stained in
green which indicated the cells were alive. Alginate lyase was used to dissolve the
alginate shells in which, the intact microtissues was released. The microtissues obtained
were characterised by a rough and uneven surface could be due to the extracellular
matrix proteins adjoining the cells. The cells of microtissues were viable and able to
proliferate and spread into 2D monolayer in replating experiment. The flicking system
has produced microbeads with controllable size and allows the growth of microtissues.
HaCaT and ORL-48 cells encapsulated in calcium alginate microbeads can integrate into
microtissues after two weeks of culture.
ix
ABSTRAK
Pengkulturan sel pada substrat yang satah menghasilkan mikrotisu yang rendah.
Pelbagai mikroteknologi diperkenalkan dan dibangunkan untuk merangkumi sel untuk
menghasil mikrotisu. Namun, pada masa ini teknologi kawalan saiz mikrokapsul untuk
sel enkapsulasi adalah mencabar. Dalam kajian ini, kami mencadangkan satu teknik
yang mudah lagi berkesan untuk merangkumi sel untuk pertumbuhan mikrotisu yang
mempunyai potensi dalam kegunaan penilaian ubat. Teknik yang terlibat dengan
pembangunan sistem jentik boleh digunakan untuk merangkumi sel dalam mikromanik
kalsium alginat pada kadar aliran dan kelajuan jentik yang berbeza. Saiz mikromanik
meningkat dengan kadar aliran tetapi menurun dengan kelajuan jentik. 80 rpm kelajuan
jentik dan 4 µl/min kadar aliran telah digunakan dalam pengkapsulan sel. Sel yang
terkandung dalam mikromanik pada kepadatan sel 31.9 × 106
sel/ml (HaCaT) dan 94.2 ×
106
sel/ml (ORL-48) dikulturkan dan diperhatikan untuk percambahan dalam satu
tempoh masa. Mikromanik itu mempunyai permukaan yang licin dengan tekstur yang
lembut dan berliang dalam pengimejan FE-SEM. Dalam pewarnaan nukleus (DAPI),
HaCaT dan ORL-48 sel yang terkandung dalam mikromanik membesar daripada
berselerak sel individu jadi sel agregat dan kemudian membentuk mikrotisu. Dalam
pewarnaan sel hidup dan mati, majoriti (≈99 %) mikrotisu diternak dalam mikromanik
diwarnakan hijau yang menunjukkan sel itu masih hidup. Alginat lyase digunakan untuk
melarutkan shell alginat untuk membebaskan mikrotisu. Mikrotisu itu mempunyai sifat
permukaan yang kasar dan tidak rata mungkin disebabkan protein matriks ekstraselular
bersebelahan sel. Sel mikrotisu itu masih hidup dan mampu berkembang dan merebak
jadi ekalapis 2D dalam eksperimen pemplatan semula. Sistem jentik telah menghasilkan
mikromanik dalam saiz dikawal untuk pertumbuhan mikrotisu. Sel HaCaT dan ORL-48
boleh membentuk mikrotisu selepas dua minggu diternak dalam mikromanik alginat.
x
CONTENTS
TITLE i
DECLARATION ii
DEDICATION iii
ACKNOWLEDGEMENT iv
LIST OF ASSOCIATED PUBLICATION v
LIST OF AWARD vii
ABSTRACT viii
CONTENTS x
LIST OF TABLES xv
LIST OF FIGURES xvi
LIST OF SYMBOLS AND ABBREVIATIONS xxii
LIST OF APPENDICES xxv
CHAPTER 1 INTRODUCTION 1
1.1 Overview 1
1.2 Research background 1
1.3 Problem statement 4
1.4 Objectives of the research 5
1.5 Scope of research 5
1.6 Thesis outline 5
CHAPTER 2 LITERATURE REVIEW 7
2.1 Introduction 7
2.2 Cell and tissue 7
2.3 Human keratinocytes 10
2.4 Oral squamous cell carcinoma cell line (ORL-48) 12
xi
2.5 Extracellular matrix (ECM) and cell adhesion 13
2.6 Phases of cell growth 15
2.7 Rationale to generate 3D cells 16
2.8 Previous methods for growing 3D cells 17
2.9 Microencapsulation 19
2.10 Different methods of microencapsulation 22
2.10.1 Simple dripping 22
2.10.2 Microfluidic 22
2.10.3 Electrostatic 23
2.10.4 Vibration technique 24
2.10.5 Jet cutter 25
2.10.6 Rotating disc and rotating nozzle atomiser 27
2.10.7 The summary of different microencapsulation 29
methods
2.11 Biopolymers used for microencapsulation of cells 30
2.12 Characterisation methods 32
2.12.1 Phase contrast microscopy 32
2.12.2 Field emission scanning electron microscope 33
(FE-SEM)
2.12.3 Fourier transform infrared spectroscopy (FTIR) 35
2.12.4 4′,6-Diamidino-2-phenylindole dihydrochloride 36
(DAPI) staining
2.12.5 Live/dead viability assay 37
CHAPTER 3 METHODOLOGY 38
3.1 Introduction 38
3.2 Overview of the research methodology 38
3.3 Overall architecture of the flicking system 42
3.3.1 Design of the flicking device 46
3.3.1.1 Circuit design of the flicking device 48
3.3.1.2 Program flow for the flicking device 51
3.3.2 Design the infusion pump of the flicking 57
system
xii
3.3.2.1 Circuit design of the infusion pump 59
3.3.2.2 Program flow for the infusion pump 63
3.4 Performance assessment of the flicking system 67
3.4.1 Verify the PWM signals generated by the 67
circuit of flicking device
3.4.2 Investigate the relationship of the 67
potentiometer voltage to the PWM signals
3.4.3 Investigate the effect of PWM signals to 68
motor speed
3.4.4 Flow rate calibration of the commercial syringe 68
pump and the customised infusion pump
3.5 The setup of the flicking experiment 69
3.6 Investigating the effects of flow rate and flicking 70
speed to the size of the microbeads
3.7 Microencapsulation of cells using the developed 71
flicking system
3.7.1 Cell culture of HaCaT and ORL-48 71
3.7.2 Microencapsulation of cells and monitoring 72
3.8 Characterising the biochemistry and surface 73
structure of the microbeads
3.8.1 FTIR scanning of the calcium alginate 73
microbeads with and without cells
3.8.2 FE-SEM scanning of the calcium alginate 73
microbeads
3.9 Characterising the biochemistry properties of the 3D
microtissues 73
3.9.1 DAPI staining 73
3.9.2 Live and dead cells staining 74
3.9.3 Extraction of 3D microtissues from 74
calcium alginate
3.9.4 FE-SEM scanning of the extracted 3D 75
microtissues
3.9.5 3D microtissues replating 75
xiii
CHAPTER 4 RESULTS AND DISCUSSION 76
4.1 Introduction 76
4.2 The functions of flicking system 76
4.3 Assessment of the flicking system performance 79
4.3.1 Verification of PWM signals 79
4.3.2 The relationship of potentiometer voltage 81
to the PWM signals
4.3.3 Effect of PWM signals on motor speed 82
4.3.4 Battery level indication of the flicking 83
device
4.3.5 Flow rate calibration of the commercial 84
syringe pump (New Era NE-4002X)
4.3.6 Flow rate calibration of the customised 85
infusion pump
4.4 The effects of flow rate and flicking speed to 86
the size of microbeads
4.4.1 The effects of different flow rates to the 86
size of microbeads
4.4.2 The effects of different flicking speeds to 93
the size of microbeads
4.5 Microencapsulation of HaCaT and ORL-48 cells 98
at different cell densities
4.5.1 HaCaT cells encapsulation at a cell density 98
of 1.75 × 106 cells/ml
4.5.2 HaCaT cells encapsulation at cell density 99
of 31.9 × 106 cells/ml
4.5.3 ORL-48 cells encapsulation at cell density 101
of 3.97 × 106 cells/ml
4.5.4 ORL-48 cells encapsulation at cell density 102
of 94.2 × 106
cells/ml
4.6 The biochemistry and surface structure of 104
the microbeads
4.6.1 The functional groups of the microbeads 104
with and without cells
xiv
4.6.2 The surface morphology of the microbeads 107
4.7 The biophysical properties of the 3D microtissues 108
4.7.1 Nucleus staining of the encapsulated 108
HaCaT and ORL-48 cells
4.7.2 The viability of the encapsulated 111
HaCaT and ORL-48 cells
4.7.3 3D microtissue extracted from calcium 112
alginate microbeads
4.7.4 The surface morphology of the 3D 113
microtissues
4.7.5 Spread of cells in microtissue replating 115
experiment
CHAPTER 5 CONCLUSION 118
5.1 Conclusion 118
5.2 Thesis contribution 119
5.3 Recommendations for future work 119
REFERENCES 121
APPENDIX 134
VITA 151
xv
LIST OF TABLES
2.1 Summary of 3D cell culture systems 18
2.2 Application of encapsulation and target of encapsulation 21
2.3 Comparison of six microencapsulation techniques on their
capabilities
30
2.4 Common biopolymers used for microencapsulation of cells
and their applications
32
3.1 Establishment of experiments 41
3.2 The relationship between “mode” and communication lines
data
65
4.1 The steps for operating the flicking system 79
xvi
LIST OF FIGURES
2.1 The anatomy of human cell 8
2.2 Human body tissues 10
2.3 Layers of the epidermis 11
2.4 Monolayer of HaCaT cells cultured in a petri dish
(Scale bar: 100 µm)
12
2.5 Monolayer of ORL-48 cells cultured in a petri dish
(Scale bar: 100 µm)
13
2.6 Integrin-mediated cell adhesion to the ECM. (a) Suspension
cell adhere to the surface of ECM. (b) The structures of
ECM
14
2.7 Different phases of cell growth 15
2.8 The five main structural forms of microcapsules 20
2.9 Calcium alginate beads formation by simple dripping 22
2.10 Calcium alginate microbeads formation by microfluidic
device
23
2.11 Calcium alginate microbeads formation by electrostatic 23
2.12 Apparatus for producing calcium alginate beads by the
vibration method, comprising a syringe pump for forcing
sodium alginate solution from a syringe, a loudspeaker, and
a sine wave sound generator
24
2.13 Arrangement of nozzle and cutting tool, with 48 stainless
steel wires
25
2.14 Scheme of the cutting process 26
2.15 The setup of JetCutter technique 26
xvii
2.16 Scheme of the rotating disc and nozzle technology for bead
production
27
2.17 Bead formation by a rotating disc device 28
2.18 Bead formation by a rotating nozzle device 28
2.19 The molecular structure of calcium alginate 31
2.20 The working principal of Phase Contrast Microscope 33
2.21 FE-SEM (Jeol, JSM – 7600F) in Microelectronic and
Nanotechnology - Shamsuddin Research Center, Universiti
Tun Hussein Onn Malaysia
34
2.22 A FTIR spectrometer (Perkin Elmer Spectrum 100) 35
2.23 Chemical structure of 4'-6-diamidine-2-phenylindole
(DAPI) dichloride
36
3.1 Flow chart of research methodology 40
3.2 Two major parts of the flicking system 42
3.3 The architecture sketchup of the flicking system (front side) 42
3.4 The architecture sketchup of the flicking system (back side) 43
3.5 Control panel of the flicking system 44
3.6 Infusion pump of the flicking system 44
3.7 Flicking device of the flicking system 45
3.8 The block diagram of flicking device circuit 46
3.9 The layout of the flicking device and controller circuit 47
3.10 The flicking device was used with a conventional syringe
pump (New Era NE-4002X) to generate Ca-Alg microbeads
during the preliminary work
47
3.11 The overall schematic diagram of the flicking device 50
3.12 Programming flow chart of the flicking device 52
3.13 Coding of custom character 1, head of battery bar (filled) 53
3.14 Coding of custom character 2, head of battery bar (hollow) 53
3.15 Coding of custom character 3, middle of battery bar (filled) 53
3.16 Coding of custom character 4, middle of battery bar
(hollow)
54
xviii
3.17 Coding of custom character 5, end of battery bar (filled) 54
3.18 Coding of custom character 6, end of battery bar (hollow) 54
3.19 Coding to read the remaining battery level 55
3.20 Coding to read the communication data from the Arduino of
infusion pump
56
3.21 Coding to start or stop the flicking device 57
3.22 The block diagram of infusion pump circuit 58
3.23 The preliminary design of the infusion pump with a
temporary casing
59
3.24 The overall schematic diagram of the infusion pump 60
3.25 The communication connections between Arduino ARD1
(flicking device) and Arduino ARD2 (infusion pump)
62
3.26 Programming flow chart of the infusion pump 64
3.27 Coding used to select the speed of infusion pump 65
3.28 Coding used to create the low, middle and high pulse
frequency and output the speed of infusion pump to the
flicking device for display on the LCD
66
3.29 The experimental setup to generate calcium alginate
microbeads
70
4.1 Front view of the flicking system prototype 77
4.2 Top view of the flicking system prototype 77
4.3 Flicking motor of the flicking system prototype 78
4.4 LCD display of the flicking system prototype 78
4.5 The output signals of PWM at different duty cycles: (a) 0 %
duty cycle, (b) 25 % duty cycle, (c) 50 % duty cycle, (d) 75
% duty cycle and (d) 100 % duty cycle
80
4.6 The relationship between the potentiometer input voltage
and duty cycle of PWM signal
81
4.7 Graph of motor speed versus duty cycle of PWM 82
4.8 (a) High, (b) middle, (c) low and (d) extremely low battery
levels
83
xix
4.9 Syringe pump (New Era NE-4002X) flow rates verification
result
84
4.10 Customised infusion pump flow rates verification 85
4.11 One of the microbeads sample generated by flow rates: (a)
5, (b) 10 and (c) 15 µl/min (Scale bar: 100 µm)
87
4.12 The size distribution graph of microbeads produced at
different flow rates of (a) 5, (b) 10 and (c) 15 µl/min
88
4.13 Size distribution of calcium alginate microbeads in different
flow rates (5, 10, 15 µl/min)
89
4.14 Some of the microbeads sample generated by flow rates: (a)
2 µl/min, (b) 4 µl/min, (c) 6 µl/min, (d) 8 µl/min and (e) 10
µl/min (Scale bar: 200 µm)
91
4.15 The size distribution graph of microbeads produced at
different flow rates of (a) 2, (b) 4, (c) 6, (d) 8 and (e) 10
µl/min
92
4.16 Size distribution of calcium alginate microbeads in different
flow rates (2, 4, 6, 8, 10 µl/min)
93
4.17 Some of the microbeads sample generated by flicking
speeds: (a) 60, (b) 70, (c) 80, (d) 90 and (e) 100 rpm (Scale
bar: 200 µm)
95
4.18 The size distribution graph of microbeads produced at
different flicking speed of (a) 60, (b) 70, (c) 80, (d) 90 and
(e) 100 rpm
96
4.19 Size distribution of calcium alginate microbeads in different
flicking speeds
97
4.20 HaCaT cells in calcium alginate with cell density of 1.75 ×
106
cells/ml after: (a) day 1, (b) day 3 and (c) day 6 of
culture (Scale bar: 100 µm)
98
4.21 HaCaT cells protrusion from the microbead (Scale bar: 100
µm)
99
xx
4.22 HaCaT cells in calcium alginate with cell density of 31.9 ×
106 cells/ml after: (a) day 1, (b) day 3, (c) day 5, (d) day 7,
(e) day 9, (f) day 11, (g) day 13 and (h) day 15 of culture
(Scale bar: 100 µm)
100
4.23 ORL-48 cells in calcium alginate with cell density of 3.97 ×
106 cells/ml after: (a) day 1, (b) day 3 and (c) day 6 and (d)
day 9 of culture (Scale bar: 100 µm)
101
4.24 ORL-48 cells in calcium alginate with cell density of 94.2 ×
106 cells/ml after: (a) day 1, (b) day 3, (c) day 5, (d) day 7,
(e) day 9, (f) day 11, (g) day 13 and (h) day 15 of culture
(Scale bar: 100 µm)
103
4.25 FTIR spectra of (a) calcium alginate, (b) HaCaT cells and
(c) calcium alginate encapsulated with HaCaT cells
106
4.26 Morphology image of calcium alginate microbead with
different magnification: (a) ×150 (Scale bar: 100 µm), (b)
×300 (Scale bar: 10 µm) and (c) ×10000 (Scale bar: 1 µm)
107
4.27 DAPI staining on HaCaT cells in calcium alginate: (a) after
3 days cultured (white light), (b) after 3 days cultured
(fluorescence), (c) after 9 days cultured and (d) after 15
days cultured. (Scale bar: 100 µm)
109
4.28 DAPI staining on ORL-48 cells in calcium alginate: (a)
after 3 days cultured, (b) after 9 days cultured and (c) after
15 days cultured. (Scale bar: 100 µm)
110
4.29 Live and dead staining on 3D HaCaT cells encapsulated in
calcium alginate microbead: (a) sample 1 and (b) sample 2.
(Scale bar: 100 µm)
112
4.30 The images of microtissues after extraction: (a) HaCaT
microtissue before and (b) after alginate lyased, (c) ORL-48
microtissue before and (d) after alginate lyased (Scale bar:
100 µm)
113
4.31 FE-SEM image of 3D HaCaT microtissue with different 114
xxi
magnifications: (a) ×150 (Scale bar: 100 µm), (b) ×300
(Scale bar: 10 µm) and (c) ×1500 (Scale bar: 10 µm)
4.32 FE-SEM image of 3D ORL-48 microtissue with different
magnifications: (a) ×150 (Scale bar: 100 µm), (b) ×300
(Scale bar: 10 µm) and (c) ×1500 (Scale bar: 10 µm)
115
4.33 Monitoring of replated 3D HaCaT microtissue on: (a) day 1,
(b) day 2, (c) day 3 and (d) day 4 (Scale bar: 100 µm)
116
4.34 Monitoring of replated 3D ORL-48 microtissue on: (a) day
1, (b) day 2, (c) day 3 and (d) day 4 (Scale bar: 100 µm)
117
xxii
LIST OF SYMBOLS AND ABBREVIATIONS
% - Percent sign
- Pulse duration
oC - Degree Celsius
2D - Two dimensional
3D - Three dimensional
BSC - Biological safety cabinet
Ca-Alg - Calcium alginate
cm - Centimeter
CO2 - Carbon dioxide
DAPI - 4′,6-Diamidino-2-phenylindole dihydrochloride
DC - Direct current
DMEM - Dulbecco‟s modified eagle medium
DNA - Deoxyribonucleic acid
ECM - Extracellular matrix
ER - Endoplasmic reticulum
ETFE - Ethylene tetrafluoroethylene
EthD-1 - Ethidium homodimer-1
FDA - Food and Drug Administration
FE-SEM - Field emission scanning electron microscope
FITC - Fluorescein isothiocyanate
FTIR - Fourier transform infrared spectroscopy
H & E - Hematoxylin and eosin
HA - Hyaluronic acid
HaCaT - Human keratinocyte
xxiii
HBSS - Hank‟s balanced salt solution
Hz - Hertz
kg-cm - Kilogram per centimeter
LABE - Low Angle Backscatter Imaging
LCD - Liquid crystal display
LEI - Lower Secondary Electron Image
MiNT-SRC - Microelectronic and Nanotechnology –
Shamsuddin Research Center
mg/ml - Miligram per mililiter
min - Minute
ml - Mililiter
mm - Milimeter
nm - Nanometer
ORL-48 - Oral squamous cell carcinoma cell line
OSCC - Oral squamous cell carcinoma
PAA - Poly(acrylic acid)
PAam - Polyacrylamide
PCB - Printed circuit board
PCL - Poly(ε-caprolactone)
PDMAEM - Poly(dimethylaminoethylmethacrylate) hydrochloride
PEG - Poly(ethylene glycol)
PGA - Polyglycolide
PLA - Polylactide
PLAGA - Poly(lactic acid-glycolic acid)
PLGA - Poly(l-lactide-co-glycolide)
PLLA - Poly(L-lactic acid)
PMMA - Polymethylmethacrylate
PNIPAAm - Poly(N-isopropylacrylamide)
PPF - Poly(propylene fumarate)
xxiv
PWM - Pulse width modulation
RNA - Ribonucleic acid
rpm - Revolutions per minute
SD - Standard deviation
SEI - Secondary Electron Image
SEM - Scanning electron microscope
µl - Microliter
µl/min - Microliter per minute
µm - Micrometer
µM - Micromolar
UK - United Kingdom
US - United States
USA - United States of America
UTHM - Universiti Tun Hussein Onn Malaysia
V - Volt
w/v - Weight per volume
xxv
LIST OF APPENDICES
APPENDIX TITLE PAGE
A Arduino source code of the flicking device 134
B Arduino source code of the infusion pump 145
C List of hardware used and specification 149
1. CHAPTER 1
INTRODUCTION
1.1 Overview
Microbeads or microcapsules have wide applications in biomedical engineering field
that include drug delivery, encapsulation of biomolecules, tissue padding and tissue
regeneration. General information concerning microbeads or microcapsules is briefly
illustrated in the research background. The problem statement highlights the weakness
of current methods to fabricate microbeads. Consequently, a method which is very
simple, reliable and uses cheap materials available in the lab was introduced to generate
microbeads. Nonetheless, this chapter also covers the objectives of the research, scope of
research and thesis outline.
1.2 Research background
In the development of tissue engineering, technologies for creating living functional
tissues in the laboratory are being developed and discovered. Tissue engineering is an
alternative to organ transplantation, drug therapy and gene therapy [1]. Animal models
used for drug testing and drug discovery studies are not encouraged due to ethical and
feasibility issues. Thus, in vitro tissue models (self cultured microtissues) are actively
used in research as an alternative for quantitative, repetitive and systematic investigation
of drugs in order to reduce the usage of animal models. These tissue models can be used
2
for high-throughput screening of drugs and for pharmacokinetic analyses of drugs [2].
For example, one man was brain dead and another five people were in hospital after an
experimental drug was administered to 90 people in a French clinical trial, as reported
by British Broadcasting Corporation (BBC) on 15 January 2016. This incident revealed
the vital of using alternative tissue models with more availability for experimental drug
trial might avoid sacrifice of life.
Various in vitro methods had been developed to culture microtissues. The most
common method to culture microtissue is culturing cells on scaffolds of biopolymers
that can be produced using electrospinning, salt leaching and ice particle leaching
method [3]. With this method, the cells are scattered in the pores of the scaffolds.
Culturing cells on a planar compliant substrate such as a hydrogel produces low yield
and inconsistent size of microtissues. This technique is arguably because it is different
from the actual biological microenvironment in the tissue [4]. Alternatively, microtissue
can be cultured by using microencapsulation technique that allows a compound (cells) to
be encapsulated inside a tiny spheroid known as microsphere or microbead, having an
average diameter as small as one micro meter to several hundred micro meters [5].
Microencapsulation of cells in the calcium alginate microbeads is leading to the
formation of microtissues (multicellular spheroids) [6, 7]. The unique advantage of this
technique is that cell culture is performed within a 3D environment that completely
surrounds cells and enabling the delivery of intense signals to cells from all directions
[8]. Compared to the 2D monolayer cell culture, 3D microtissue models mimic the cell
structural organisation in the in vivo system and the cellular microenvironment
established in the 3D models often plays a more significant role in cellular responses to
drugs and disease progression [2].
Among the previous methods, microencapsulation of cells is a promising method
because microencapsulation leads to the formation of living microtissues which is
suitable to be used for therapeutic tests. Microbeads or microcapsules have wide
applications in biomedical engineering field that include drug delivery, encapsulation of
biomolecules, tissue padding and tissue regeneration. The selection of a suitable
encapsulating material with appropriate porosity, which can facilitate the transport of
nutrients, proteins and drugs while blocking attack of antibodies and bacteria is critical
3
[9]. The capsule must be mechanically stable and easy to handle. These requirements
may be fulfilled by controlling the size and thickness of the encapsulating polymer
membrane at microscale range.
Microcapsules are spherical particles containing a core substance with the size
varying between 50 nm to 2 mm [10]. During the early days in the 80‟s,
microencapsulation technologies were used for the microencapsulation of drugs and
liquidified food [11, 12]. Later in the 90‟s, this technology was discovered with new
application in tissue engineering [13]. In tissue engineering, microcapsules of sodium
alginate for microencapsulation of cells have the potential for the application in
immunoisolatory and biochemical assays [14]. Biomaterials for microencapsulation of
cells play a major roll to determine the fate of the cells encapsulated and also the
proliferation of cells. There are various types of materials used to produce microcapsules
such as agarose, collagen, alginate, chitosan and gelatin [15]. Sodium alginate has been
found suitable for biotechnology and biomedical applications mainly as a material for
the encapsulation of different cells for biochemical processing and immunoisolatory
while the cells can still maintain viability within the hydrogel [14]. It has been employed
for encapsulating cells to be transplanted, since it is biocompatible both to the host and
enclosed cells [8].
Some of the popular methods developed particularly for the microencapsulation
of cells are the microfluidic device [16], emulsification [17], extrusion, electrospray
[18], electrostatic [19-21] and airflow [22]. However, these methods are complex in
design [23], required high voltage supply [20], post cleaning process [24] and large
volume of reagents. The purpose of this research is to develop a novel flicking system
that could be used to produce uniform and controllable sized of calcium alginate
microbeads for 3D cells encapsulation. Calcium alginate was proposed to be used for
encapsulation of cells is because this biomaterial is non-toxic, degradable and it is a
biocompatible material approved by US Food and Drug Administration (FDA) [9, 25].
Under the FDA approval, calcium alginate is permitted to be an implantable material in
the human body [9, 25]. The contribution of this study is expected to be useful for
generating 3D cells model for studying therapeutic cytochemicals. The biochemistry
properties of the microbeads and biophysical properties of the microtissues formed will
4
be characterised using microscopy observation, FTIR scanning, Field Emission
Scanning Electron Microscope (FE-SEM), DAPI staining, live and dead stainings and
3D microtissues replating. The backbone of this study is to be useful for generating the
3D microtissues, which is identified to be relevant to drive major innovations in tissue
engineering.
1.3 Problem statement
The microbeads of calcium alginate can be easily generated by extruding droplets of
sodium alginate solution in air using a syringe and allowed to polymerised in the
calcium chloride solution. However, the extrusion technique provided limited control
over the size of the microbeads and usually large beads of calcium alginate in millimeter
size were produced. Small calcium alginate beads in a few hundreds of micron are
desirable because this range of microbeads provide higher mechanical strength, easier
implantation, better transport of oxygen and nutrients for the cells [26]. Although
alginate beads can be fabricated by using microfluidic approach in micron size, the
alginate microbeads formed based on microemulsion technique were covered with oil
film and hence, post cleaning process is required to remove the oil film before
incubating the cells. The oil film can be sealing the gas from the cells in encapsulation.
Strong mechanical and chemical treatments are required to remove the immiscible fluid,
which prolongs exposure of the cells to divalent ions or solvents which may harm and
kill the cells [27]. Other methods such as microextrusion techniques assisted by
electrostatic field and electrospraying were shown to decrease the alginate drop size.
However, these methods required sophisticated high power circuit to create atomization
of alginate droplets which is dangerous with electric shock hazard [20, 28].
Based on the literature review, a simple yet efficient technique could be
designed and developed to address the several issues raised for current techniques of
microencapsulation. Hence, the purpose of this study is to develop a novel flicking
system that could be used to produce calcium alginate (Ca-Alg) microbeads for the
microencapsulation of cells. The flicking method used by the flicking system to
encapsulate cells is simple and highly reproducible.
5
1.4 Objectives of the research
The aim of the research is the development of a flicking system for producing 3D cells
in microbeads leading to the growth of microtissues. Four objectives were outlined to
achieve the aim:
a) To develop a flicking system to produce calcium alginate microbeads size in
200 to 300 micron.
b) To investigate the effects of infusion pump flow rates and flicking motor
speed to the size of the microbeads produced.
c) To microencapsulate cells using the developed flicking system.
d) To characterise the biophysical properties of the 3D microtissues formed in
calcium alginate microbeads.
1.5 Scope of research
This research was divided into four scopes which are:
a) Design and development of a mechatronic system of microextrusion system
with a flicking device (flicking system).
b) Determining the syringe flow rates and flicking speed of the system to
encapsulate cells in the appropriate microbeads size.
c) Encapsulating human keratinocyte cell lines (HaCaT) and oral squamous cell
carcinoma (ORL-48) cells in the calcium alginate microbeads.
d) Monitoring the growth of the microencapsulated cells into microtissues.
1.6 Thesis outline
This thesis was divided into five chapters. Chapter 1 introduced an overview of the
research background, problem statement, objectives of the research, scope of research
6
and thesis outline. Chapter 2 revealed the cells type, the method used in
microencapsulation, biopolymers used for microencapsulation of cells, rationale to
generate 3D cells, instrument utilised in the research and stainings used to characterise
the biophysical of 3D microtissues. Chapter 3 outlined the experiment procedure of this
research including the materials and methods used in the development of flicking
system, experimental setup, investigating the effects of flow rates and flicking speed to
the size of microbeads, characterising the biochemistry and surface structure of the
microbeads, preparation for microencapsulation of cells using the developed flicking
system and characterising the biophysical properties of the 3D microtissues formed from
the 3D cells. Chapter 4 presented the results and discussion of the research project which
included the functions of flicking system, assessment of the system performance, the
effects of flow rates and flicking speed to the size of microbeads, the biochemistry and
surface structure of the microbeads, microencapsulation of HaCaT and ORL-48 cells at
different cell densities and the biophysical properties of the 3D microtissues. At last but
not least, Chapter 5 delivered the conclusion, thesis contribution and recommendations
for future work.
2. CHAPTER 2
LITERATURE REVIEWS
2.1 Introduction
This chapter has included the summarised information of the relevant studies on cells
microencapsulation leading to microtissues formation in the calcium alginate
microbeads. The literature review covered the fundamental knowledge of cell and tissue,
microencapsulation techniques and techniques used for biophysical characterisation of
microtissues are discussed in the following subchapters which are cell and tissue,
extracellular matrix (ECM), cell adhesion, phases of cell growth, microencapsulation,
different technology of microencapsulation, biopolymer used for microencapsulation of
cells, rationale to generate 3D cells, inverted phase contrast microscopy, field emission
scanning microscope (FE-SEM), fourier transform infrared spectroscopy (FTIR), DAPI
staining and live/dead viability assay.
The sources of the literatures reviewed are journals, articles, and information
from books and internet, which are important on identifying problems as well as give
ideas in this research.
2.2 Cell and tissue
The cell is the fundamental structural, functional, and biological unit of all known living
organisms. Cells are the smallest unit of life that can replicate freely. Cells consist
8
of cytoplasm enclosed within a membrane, which contains many biomolecules such
as nucleic acids and proteins [29]. Organisms can be classified as unicellular (cell and
bacteria) or multicellular (plants and animals). Human has about 100 trillion (1014
) cells
while the number of cells in plants and animals varies from species to species [30]. Most
animal and plant cells are in dimensions between 1 and 100 micrometres and only can be
visible under the microscope [31]. The cells build the structure of body, consume
nutrients from food, convert those nutrients into energy, and carry out specialist
functions. Organelles are structures that perform specialised tasks within the cell. These
organelles containing in the cytoplasm are such as pinocytotic vesicle, golgi vesicles,
cytoskeleton, endoplasmic reticulum (ER), golgi apparatus, lysosomes, mitochondria,
centrioles, microtubules, nucleus, nucleolus, plasma membrane and ribosomes as shown
in Figure 2.1.
Figure 2.1: The anatomy of human cell [32]
Centriole
(within
centrosome)
Lysosome
Golgi
apparatus
(Golgi body)
Nucleus
Nucleus membrane
Genetic material
(DNA)
Nucleolus
Endoplasmic
reticulum
Ribosomes
Plasma
membrane
(cell
membrane)
Cytoplasm
Mitochondrion
9
Cytoplasm is a jelly-like fluid which surrounds the cell‟s organelles and nucleus.
The cytoskeleton is a chain of long fibers that build up the cell‟s structural framework
that has several critical functions, allowing cells to move, cell division and determining
cell shape. In addition, cytoskeleton provides a track-like system that directs the
movement of organelles and other substances within cells. The endoplasmic reticulum is
responsible in molecule processing and transport to their specific destinations either
outside or inside the cell. Nonetheless, the golgi apparatus is responsible in packaging
molecules for export from the cell. Lysosomes destroy toxic substances and recycle
exhausted cell parts. In addition, mitochondria provide the energy for cells to replicate
themselves with their own genetic material. Ribosomes use the cell‟s genetic
instructions to make proteins at the same time. Besides that, the nucleus contains most of
the cell‟s genetic material such as RNA (ribonucleic acid) and DNA (deoxyribonucleic
acid). The plasma membrane is the outer most layer which enclosed the cell and allows
the transport of materials to leave and enter the cell.
Tissue is an assembly of cells with similar characteristics which performs a
specific function. Different types of tissues can be found in different organs as shown in
Figure 2.2. Organs are made of tissues that provide the various functions of organs
required to maintain biological life. There are four basic types of tissue in human, which
are connective, epithelial, nervous and muscular tissue. The function of connective
tissue supports and binds with other tissues. Connective tissue cells can be found in a
large amount of extracellular matrix (ECM). Epithelial tissue covers the body surface
and forms the lining for most internal cavities of organs. Epithelial tissues have different
cells shapes which are squamous, cuboidal and columnar epithelium. The main functions
of epithelial tissue are filtration, protection secretion, and absorption of glucose from the
lumen of the intestine. Skin is one of the organs that consist of most epithelial tissue
which protects the body from bacteria, dirt and microbes that may be harmful.
10
Figure 2.2: Human body tissues [33]
2.3 Human keratinocytes
The epidermis is made of squamous epithelium that forms the protective layer of the
skin [34]. Keratinocytes are the main cell type in the epidermis layer. Epidermis consists
of five histologically distinct cellular layers such as stratum corneum, stratum lucidum,
stratum granulosum, stratum spinosum and stratum basale as shown in Figure 2.3.
Stratum spinosum is the layer with the most human keratinocytes in the epidermis.
Human keratinocytes cell line (HaCaT) is transformed immortal keratinocyte cell line
with abnormal chromosomes number from adult human skin that has been widely used
for scientific research, studies of cell biology and differentiation. HaCaT cells are
Connective
tissue
Skeletal muscle
Epithelial tissue Smooth muscle
Nervous
tissue
Cardiac muscle
11
utilised for their high capacity to proliferate and differentiate in vitro [35]. HaCaT cells
have reduced tissue proliferation and regeneration compared to normal epidermal
keratinocytes [36, 37]. By the addition of growth factors can stimulate the proliferation
rate of HaCaT cells [38], the characterisation of human keratinocyte using this model
becomes reproducible and overcome the short culture lifespan issue of normal human
keratinocyte. Figure 2.4 shows a phase contrast photomicrograph of HaCaT cells in
monolayer of culture. In monolayer or 2D structure, HaCaT cells are displayed with
polygonal shape and tightly coupled to the neighbouring cells when grown into
confluency.
Figure 2.3: Layers of the epidermis [39]
Stratum corneum
Stratum lucidum
Stratum granulosum
Stratum spinosum
Stratum basale
Melanocyte
Dermis
Dead cells filled
with keratin
Lamellar granules
Keratinocyte
Merkel cell
Sensory neuron
12
Figure 2.4: Monolayer of HaCaT cells cultured in a petri dish (Scale bar: 100 µm)
2.4 Oral squamous cell carcinoma cell line (ORL-48)
Oral cancer is a common disease and silent killer in the developing country, especially in
Southeast Asia country. Microtissue models of cancer cells are necessary in drug
discovery and the cancer research. Oral squamous cell carcinoma (OSCC) cell line
(ORL-48) was established by Cancer Research Malaysia. They are surgically explanted
epithelial specimens obtained from untreated primary human oral carcinoma cell in the
squamous layer of the oral cavity. These epithelial cells were genetically modified to be
immortal and grown into monolayer with doubling times ranging between 26.4 and 40.8
hours [40]. Figure 2.5 shows a phase contrast photomicrograph of ORL-48 cells in
monolayer culture. In 2D structure or monolayer, ORL-48 cells are typically irregular
elongated polygonal shape and coupled randomly with the neighbouring cells.
13
Figure 2.5: Monolayer of ORL-48 cells cultured in a petri dish
(Scale bar: 100 µm)
2.5 Extracellular matrix (ECM) and cell adhesion
Extracellular matrix (ECM) is made up of polysaccharides and proteins, including
laminins, collagens, elastins, proteoglycans and fibronectins, all secreted by the cell
[41]. In animal cells, the ECM enclosed cells as fibrils that contact the cells [42]. Cells
in animals are also joined directly to each other by cell adhesion proteins at the cell
surface. In addition, ECM provides a biochemical barrier, mechanical support and a
medium for extracellular communication that is assisted by cell adhesion proteins,
moreover ECM provides tensile strength for tendons, compressive strength for cartilage,
hydraulic protection for cells and elasticity to the walls of blood vessels [42].
Adhesion of cells to the extracellular matrix (ECM) is key to the regulation of
cellular morphology, differentiation, proliferation, migration and survival [43]. These
functions are necessary during tissue development, maintenance of tissue structure and
the initiation of tissue repair. Integrins are the main receptors that moderate cell
adhesion to the components of ECM [44, 45]. Figure 2.6(a) shows a suspension cell
adhesion to ECM proteins via integrins and Figure 2.6(b) shows the structures of ECM
which consist actin cytoskeleton, integrin receptors, adhesion proteins and focal
adhesion complexes. Integrins are categorised as the heterodimers which consisted of
14
two different chains, the α (alpha) and β (beta) subunits [46]. During cell-ECM
adhesion, the specific ligands in the ECM decide the type of α and β subunits of the
integrins being attached by the cell [47]. There are numerous integrins exist on the cell
membrane and they work collaboratively with the cell adhesion proteins in cell-ECM
adhesion [48].
Figure 2.6: Integrin-mediated cell adhesion to the ECM. (a) Suspension cell adhere to
the surface of ECM. (b) The structures of ECM [49]
(a)
(b)
15
2.6 Phases of cell growth
A regular growth curve for cultured cells displayed a sigmoid pattern of proliferation.
The growth phases correlative with normal cells are divided into lag phase, logarithmic
growth phase, stationary (or plateau) phase and decline phase as shown in Figure 2.7. It
was vital to understand the growth characteristics of the cell line because any change in
cellular growth can represent a significant problem of the cell line and affect the
experimental results [50]. At lag phase, the cells do not divide but adapting to the culture
conditions and the length of this phase will depend upon the growth phase of the cell
line at the seeding density and time of subculture. During log growth phase, the cells
actively proliferate and exponentially increase in cell density. The cell population is
considered to be the most viable at this phase, therefore it was recommended to assess
cellular function at this stage. Each cell line will show different cell proliferation
kinetics during the log phase, therefore it is the optimal phase for determining the
population doubling time [50]. After the log phase, the cellular proliferation slows down
due to the cell population becoming confluent at stationary phase. Ultimately, the cell
death predominates in this death phase and there will be a reduction in the number of
viable cells. Cell death was not due to the reduction in nutrient supplements but the
natural path of the cellular cycle.
Figure 2.7: Different phases of cell growth [50]
Log N
um
ber
of
Cel
ls
Lag Log Stationary
/ Plateau Death
Live
Total
1 2 3 4 5 6 7 8 9 10 Days
16
2.7 Rationale to generate 3D cells
In the in vitro or two-dimensional (2D) culture, cells are tightly spread and coupled to
the bottom surface of culture flask which is contrarily to cells that retain in-vivo [4]. The
extracellular matrix components, cell-to-cell and cell-to-matrix interaction that are
important for proliferation, differentiation and cellular functions in vivo are lost in the
conventional 2D culture [51].
Cell to cell interaction in 2D culture is mainly concentrated at the boundary of
the flattened cells [52]. Cells grown in 2D spread involuntarily by producing limited
amount of extracellular matrix proteins due to the contactless spreading of cells [53].
The spatial organisation of the cells in 2D is distorted compared with the three-
dimensional (3D) tissue in-vivo [54].
3D cells are good models as “near-to-in vivo” systems and reveal useful insights
from a variety of ways [54]. 3D cell model is a cost effective screening platform for drug
development and testing, simultaneously provides a better and more realistic predictive
value for risk and safety assessment [54].
A major benefit of the 3D over the 2D culture is the decrease in the gap between
cell cultures system and the cellular physiology [54]. Several researches show that 3D
organisation of cells reveals more novel and surprising visions into the tumorigenesis
mechanism which could represent an integral missing component in the in vitro cancer
studies [55].
Thus, 3D cell culture is believed to have better similarity to the actual tissue
model for cancer cell research because 3D culture restore specific morphological and
biochemical features similar to the corresponding tissue in-vivo [56].
Besides that, modelling the complexity of cancer utilising these cell lines on
standard plastic substrate does not accurately represent the tumour microenvironment
[57]. However, tumour cells cultured in 2D monolayer conditions do not respond to
cancer therapeutics [57]. Thus, 3D cells culture is useful for drug testing on cancer
tumour.
Many researchers want to mimic the actual cancer tumour in human body by
culturing cancer cells into 3D cells because the 3D cells reveal a more realistic drug
17
response, precisely characterises the disease and mimics the tumour microenvironment
in human body [58]. Other than that, the applications of 3D cell are differentiation
studies, drug discovery and pharmacological applications, cancer research, gene and
protein expression studies [59].
2.8 Previous methods for growing 3D cells
3D cells culture exhibits features that are closer to the complex in vivo conditions and
the 3D culture models have proven to be more realistic for translating the study findings
for in vivo applications [59].
Various in vitro methods had been developed for growing 3D cells as shown in
Table 2.1. While each method presents its unique factors, the appropriate method must
be selected to meet the requirements for the specific type of cells in different
applications.
The most common method to culture microtissue is culturing cells in suspension
such as hanging drop method. With this method, the cells are scattered in the suspension
media with limited flexibility. It is not a safe to use when one is dealing with extremely
pathogenic organisms as the user can easily get an infection.
Matrigel, Extracel and AlgiMatrix are the common methods used to culture 3D
microtissues on substrate. Culturing cells on a planar compliant substrate produces low
yield and inconsistent size of microtissues.
Other than that, microencapsulation techniques are also applied in microtissue
culturing that allows 3D cells growing within tiny spheroid matrix. The unique
advantage of this technique is that cell culture is performed within a 3D environment
that completely surrounds cells, enabling the delivery of intense signals to cells from all
directions [8].
18
Table 2.1: Summary of 3D cell culture systems [60]
3D cell culture systems
Pros
Cons Methods
3D spheroids grown in
suspension.
No added materials
Consistent spheroid
formation; control
over size
Co-cultures possible
Transparent
High-throughput
screening capable;
compatible with
liquid handling tools
Inexpensive
No support or
porosity
Limited flexibility
Size of spheroid
limiting
Magnetic cell
levitation [4] and
hanging drop [61]
3D spheroids grown on
matrix.
Large variety of
natural or synthetic
materials
Customisable
Co-cultures possible
Inexpensive
Gelling mechanism
Gel-to-gel variation
and structural
changes over time
Undefined
constituents in
natural gels
May not be
transparent
High-throughput
screening options
limited
Hydrogel [3],
Matrigel, Extracel
and AlgiMatrix [62]
3D spheroid grown
within matrix.
Large variety of
materials possible
for desired
properties
Customisable
Co-cultures possible
Medium cost
Possible scaffold-to-
scaffold variation
May not be
transparent
Cell removal may be
difficult
High-throughput
screening options
limited
Microencapsulations
[5, 7]
Culture media
3D spheroid
Culture media
3D spheroid
Matrix
Matrix
3D spheroid
Culture media
19
2.9 Microencapsulation
Vincenzo Bisceglie was the first to encapsulate cells using polymer membranes in 1933
[63]. Based on Bisceglie‟s work, Thomas Chang proposed the idea of encapsulating
cells within ultra thin polymer membrane microcapsules to provide immunoprotection to
the cells and introduced the term "artificial cells" to define this concept of
bioencapsulation in 1964 [64]. Microcapsule, microsphere or microbead are similar
terms that is defined as a spherical particle containing a core substance with a size
between 50 nm to 2 mm [10]. However, microcapsules may not be spherical structurally
but are referred to empty particles made of hydrogel (Figure 2.8). Many researches were
worked on microspheres and microcapsules for the applications of controlled drug
release formulations. They have been proven suitable for many applications which can
be produced from natural or synthetic materials, but they are usually found in nature, for
example, microencapsulation is also a natural phenomenon as what we can observe in
the bacterial spores, plants seeds and egg shells [65].
Microcapsules are divided into three categories that are determined by the
structure and layers of encapsulation. Mononuclear or single-core (Type A) is the
simplest form of microcapsules. The core material of mononuclear microcapsules
usually is a liquid, thus they can be called as liquid-core microcapsules also which is
surrounded by a layer of membrane [66]. The diameter of the core material and the
membrane thickness can vary in size. Multi-shells (Type B) microcapsules have multiple
shell layers which modify the original permeability and stability characteristics of the
microcapsules [67]. Polynuclear or multi-core (Type C) microcapsules containing two or
more individual cores [68]. Microcapsules of Type A-C are normally looked like
spherically shaped particles with a well-defined shell and core structure but other non-
spherical forms of microcapsules are categorised as Type D and Type E of
microcapsules. Type D microcapsule is the most common type of microcapsules without
multilayer of membrane applied for encapsulation of cells, particles and does not possess
multiple layer of membrane. We always referred these microcapsules as microbeads or
microspheres [69]. In addition, Type E are non-spherical or irregular shaped
20
microcapsules that can be polynuclear, mononuclear or solid particle encapsulation and
they are commonly used in the pharmaceutical and food industry [70].
Figure 2.8: The five main structural forms of microcapsules [65]
The microencapsulation technology has been applied to biotechnological and
medical disciplines recently such as the encapsulation of mammalian cells [71],
implantation of cells [72] and encapsulation of recombinant therapeutic proteins [73].
There are six main applications of microencapsulation within a membrane compared to
its non-encapsulated form as shown in Table 2.2 with the examples of where the process
was implemented.
A. Single-core B. Multi-shell C. Multi-core
D. Entrapment E. Irregular
21
Table 2.2: Application of encapsulation and target of encapsulation [65] [65]
Application of encapsulation Target of encapsulation
Protection or stabilization of the encapsulant from
interactions with reactive environments or future
surroundings
Cells (Prevention)
Mammalian (immuno-response and cell damage
due to agitation and aeration)
Yeast (ethanol toxicity)
Enzymes
Improved stability and reactivity
Prevent denaturing
Food additives and bioactives
Off-setting loss and deterioration by:
High temperature food processing
passage through the GI tract
hygroscopicity
evaporation (aroma compounds)
oxidation
Recombinant proteins
Improved stability and protection
Sustained, controlled or timed release of the core
material Agrochemicals (delivery of fertilizers, repellents,
herbicides, fungicides, etc.)
Folic acid (controlled release)
Pharmaceuticals (controlled delivery)
Antibody (sustained release)
Adhesive (dispensed upon pressure)
Butan-1-ol flavour (delayed release)
Fragrances (dispensed upon pressure)
Targeting of encapsulated compounds to specific
sites DNA to phagocytic cells
Vitamin C (oral route)
Probiotic bacteria (intestine)
Doxycycline for localized treatment of septic
arthritis
Enabling core material to be used as an extraction
device for product removal including in situ
product recovery
Environmental pollutants
Extraction of pharmaceuticals,
herbicides/pesticides and heavy metals from water
In situ product recovery
Culture environments
Recovery of primary and secondary metabolites
Bioconversion processes
Removal of products from hydrolysis of Penicillin
G and a lipase-catalysed reaction
Improved flow properties of the encapsulant for
enhanced handling, usage and storage including
safety
Pesticides (enhanced safety handlng and usage)
Biosorbents (improved usage and storage)
Enzyme (better storage)
Bioactives (enhanced handling and storage)
Hydrophobic liquids (new applicability)
Improved organoleptic properties of the
encapsulation product Shark liver oil (preventing undesirable taste)
Tea bags (improved appearance)
Antibiotic colistin (hiding taste)
Ultra Rice (preventing undesirable appearance
and taste)
22
2.10 Different methods of microencapsulation
2.10.1 Simple dripping
Calcium alginate beads can be easily generated by extruding drops [74] of sodium
alginate solution in the air using a syringe and collecting the droplets of sodium alginate
into calcium chloride solution, it offers little control over drop formation and large
calcium alginate beads in millimeter size were produced as shown in Figure 2.9.
Figure 2.9: Calcium alginate beads formation by simple dripping
2.10.2 Microfluidic
Microfluidic device can be used to produce small calcium alginate microbeads in a few
hundred micron size (nanometric size is also possible) with the aid of dispersion oil to
disperse the alginate solution into small droplets as shown in Figure 2.10. Although this
method produced smaller alginate drops, the precise control over the gelation process is
complicated and the removal of the immiscible fluid (oil) requires strong chemical and
mechanical treatments, which prolongs exposure of the cells to solvents which will be a
threat to the cells [27].
Alginate droplet
Calcium chloride
solution
Calcium alginate
bead
Syringe
Alginate solution
Syringe needle
23
Figure 2.10: Calcium alginate microbeads formation by microfluidic device
2.10.3 Electrostatic
Alternatively, microbeads generation techniques assisted by electrostatic field and
electrospray could decrease the size of the alginate droplets as shown in Figure 2.18. In
this method, the high voltage (up to 25 kV) of electricity in either static or pulse is used
to create the electrostatic potential between the needle and the hardening bath (calcium
chloride) in order to disperse the alginate solution into small droplets [20, 28]. This
method is able to produce smaller microbeads (≥ 50 μm in diameter) under sterile
conditions with uniform size and shape under reproducible conditions compared to
normal dripping method [75].
Figure 2.11: Calcium alginate microbeads formation by electrostatic
Oil
Oil
Oil Alginate
Alginate droplets
Syringe
Alginate solution
Syringe needle
High voltage
Alginate droplet
Calcium chloride
solution
Calcium alginate
bead
24
2.10.4 Vibration technique
The vibration technique is the most sophisticated dropping technique for
microencapsulation. Vibration nozzle was used to produce alginate beads with
immobilised proteins [76]. The vibration technique used mechanical vibrations
generated by speaker to break up a jet of cell-alginate mixture into uniform droplets as
shown in Figure 2.12. The calcium alginate bead size is controlled by varying the jet
velocity, vibration frequency and jet diameter [76]. The main disadvantage of vibrating
technique is low production yields of small microbeads, as it only produce a single
droplet, one after another at once. The production flow rate is mainly dependent on the
nozzle diameter with increasing diameter resulting in higher production rate, however
the production rate is still low for the largest nozzle diameter [75].
Figure 2.12: Apparatus for producing calcium alginate beads by the vibration method,
comprising a syringe pump for forcing sodium alginate solution from a syringe, a
loudspeaker, and a sine wave sound generator [76]
Wood
board
Syringe pump
Syringe
Sodium alginate solution
with protein
100% Isoamyl
alcohol
50% CaCl2 aq and 50%
Isopropyl alcohol
mixture
Speaker
Sine wave sound
generator
REFERENCES
[1] W. M. Saltzman. Tissue Engineering: Engineering Principles for the Design of
Replacement Organs and Tissues. Oxford: Oxford University Press. 2004.
[2] N. T. Elliott and F. Yuan. A review of three-dimensional in vitro tissue models
for drug discovery and transport studies. Journal of Pharmaceutical Sciences.
2011. 100(1): 59-74.
[3] B. Dhandayuthapani, Y. Yoshida, T. Maekawa, and D. S. Kumar. Polymeric
Scaffolds in Tissue Engineering Application: A Review. International Journal of
Polymer Science. 2011. 2011: 19.
[4] G. R. Souza, J. R. Molina, R. M. Raphael, M. G. Ozawa, D. J. Stark, C. S. Levin,
et al. Three-dimensional tissue culture based on magnetic cell levitation. Nature
Nanotechnology. 2010. 5(4): 291-6.
[5] T. C. S. Rama Dubey, K.U. Bhasker Rao. Microencapsulation Technology and
Applications. Defence Sci J. 2009. 59(1): 82-95.
[6] S. Sakai, S. Ito, and K. Kawakami. Calcium alginate microcapsules with
spherical liquid cores templated by gelatin microparticles for mass production of
multicellular spheroids. Acta Biomater. 2010. 6(8): 3132-7.
[7] S. C. Wong, C. F. Soon, W. Y. Leong, and K. S. Tee. Flicking technique for
microencapsulation of cells in calcium alginate leading to the microtissue
formation. J Microencapsul. 2016. 1-10.
[8] I. Ghidoni, T. Chlapanidas, M. Bucco, F. Crovato, M. Marazzi, D. Vigo, et al.
Alginate cell encapsulation: new advances in reproduction and cartilage
regenerative medicine. Cytotechnology. 2008. 58(1): 49-56.
[9] G. A. Paredes Juarez, M. Spasojevic, M. M. Faas, and P. de Vos. Immunological
and technical considerations in application of alginate-based microencapsulation
systems. Frontiers in Bioengineering and Biotechnology. 2014. 2: 26.
[10] M. N. Singh, K. S. Hemant, M. Ram, and H. G. Shivakumar.
Microencapsulation: A promising technique for controlled drug delivery.
Research in Pharmaceutical Sciences. 2010. 5(2): 65-77.
122
[11] Y. Kawashima, T. Niwa, T. Handa, H. Takeuchi, T. Iwamoto, and K. Itoh.
Preparation of controlled-release microspheres of ibuprofen with acrylic
polymers by a novel quasi-emulsion solvent diffusion method. Journal of
Pharmaceutical Sciences. 1989. 78(1): 68-72.
[12] J. D. Dziezak. Microencapsulation and encapsulated ingredients. Food
Technology. 1988. 42(4): 136-51.
[13] M. Löhr, Z. Bago, H. Bergmeister, M. Ceijna, M. Freund, W. Gelbmann, et al.
Cell therapy using microencapsulated 293 cells transfected with a gene construct
expressing CYP2B1, an ifosfamide converting enzyme, instilled intra-arterially
in patients with advanced-stage pancreatic carcinoma: a phase I/II study. Journal
of molecular medicine (Berlin, Germany). 1999. 77(4): 393-8.
[14] L. Wang, R. M. Shelton, P. R. Cooper, M. Lawson, J. T. Triffitt, and J. E.
Barralet. Evaluation of sodium alginate for bone marrow cell tissue engineering.
Biomaterials. 2003. 24(20): 3475-81.
[15] A. Kang, J. Park, J. Ju, G. S. Jeong, and S. H. Lee. Cell encapsulation via
microtechnologies. Biomaterials. 2014. 35(9): 2651-63.
[16] Y. Hu, Q. Wang, J. Wang, J. Zhu, H. Wang, and Y. Yang. Shape controllable
microgel particles prepared by microfluidic combining external ionic
crosslinking. Biomicrofluidics. 2012. 6(2): 26502-265029.
[17] K. K. Mishra, R. K. Khardekar, R. Singh, and H. C. Pant. Fabrication of
polystyrene hollow microspheres as laser fudion targets by optimized density
matched emulsion technique and characterization. Pramana-Journal of Physics.
2002. 59(1): 113-131.
[18] S. D. Nath, S. Son, A. Sadiasa, Y. K. Min, and B. T. Lee. Preparation and
characterization of PLGA microspheres by the electrospraying method for
delivering simvastatin for bone regeneration. International Journal of
Pharmaceutics. 2013. 443(1-2): 87-94.
[19] N. Li, X. X. Xu, G. W. Sun, X. Guo, Y. Liu, S. J. Wang, et al. The effect of
electrostatic microencapsulation process on biological properties of tumour cells.
Journal of Microencapsulation. 2013. 30(6): 530-7.
[20] D. Lewinska, J. Bukowski, M. Kozuchowski, A. Kinasiewicz, and A. Werynski.
Electrostatic Microencapsulation of Living Cells. Biocybernetics and Biomedical
Engineering. 2008. 28(2): 69–84.
[21] W. Zhang and X. He. Encapsulation of living cells in small ( approximately 100
microm) alginate microcapsules by electrostatic spraying: a parametric study.
Journal of Biomechanical Engineering. 2009. 131(7): 074515.
123
[22] S. Sugiura, T. Oda, Y. Aoyagi, R. Matsuo, T. Enomoto, K. Matsumoto, et al.
Microfabricated airflow nozzle for microencapsulation of living cells into 150
micrometer microcapsules. Biomedical Microdevices. 2007. 9(1): 91-9.
[23] U. Pruesse, U. Jahnz, P. Wittlich, and K.-D. Vorlop. Scale-up of the JetCutter
technology. Chemistry & Industry. 2003. 12: 636-641.
[24] K.-S. Huang, M.-K. Liu, C.-H. Wu, Y.-T. Yen, and Y.-C. Lin. Calcium alginate
microcapsule generation on a microfluidic system fabricated using the optical
disk process. Journal of Micromechanics and Microengineering. 2007. 17:
1428–1434.
[25] P. de Vos, H. A. Lazarjani, D. Poncelet, and M. M. Faas. Polymers in cell
encapsulation from an enveloped cell perspective. Advanced Drug Delivery
Reviews. 2014. 67-68: 15-34.
[26] D. Chicheportiche and G. Reach. In vitro kinetics of insulin release by
microencapsulated rat islets: effect of the size of the microcapsules.
Diabetologia. 1988. 31(1): 54-7.
[27] C. J. Martinez, J. W. Kim, C. Ye, I. Ortiz, A. C. Rowat, M. Marquez, et al. A
microfluidic approach to encapsulate living cells in uniform alginate hydrogel
microparticles. Macromolecular Bioscience. 2012. 12(7): 946-51.
[28] L. Zhang, J. Huang, T. Si, and R. X. Xu. Coaxial electrospray of microparticles
and nanoparticles for biomedical applications. Expert Review of Medical
Devices. 2012. 9(6): 595-612.
[29] B. Alberts. Cell Movements and the Shaping of the Vertebrate Body, 4th ed. New
York: Garland Science. 2002.
[30] H. Lodish, A. Berk, C. A. Kaiser, M. Krieger, M. P. Scott, A. Bretscher, et al.
Molecular Cell Biology, 6th ed. New York: W.H.Freeman and Company. 2007.
[31] N. A. Campbell, B. Williamson, and R. J. Heyden. Biology: Exploring Life.
Boston, Massachusetts: Pearson Prentice Hall. 2006.
[32] B. J. Cohen, and D. L. Wood. Memmler's The Human Body in Health and
Disease. 9th Ed. Philadelphia: Lippincott Williams & Wilkins. 2000.
[33] L. Sherwood. Fundamentals of Human Physiology. 4th Ed. USA: Brooks/Cole,
Cengage Learning. 2012.
[34] J. A. McGrath, R. A. Eady, and F. M. Pope. Rook's Textbook of Dermatology.
vol. 4, 7 ed: Blackwell Publishing, pp. 31-36; 2004.
124
[35] P. Boukamp, R. T. Petrussevska, D. Breitkreutz, J. Hornung, A. Markham, and
N. E. Fusenig. Normal keratinization in a spontaneously immortalized aneuploid
human keratinocyte cell line. The Journal of Cell Biology. 1988. 106(3): 761-71.
[36] E. Boelsma, M. C. H. Verhoeven, and M. Ponec. Reconstruction of a human skin
equivalent using a spontaneously transformed keratinocyte cell line (HaCaT).
Journal of Investigative Dermatology. 1999. 112: 489-498.
[37] K. M. Yamada and E. Cukierman. Modeling tissue morphogenesis and cancer in
3D. Cell. 2007. 130(4): 601-10.
[38] M. A. Seeger and A. S. Paller. The Roles of Growth Factors in Keratinocyte
Migration. Adv Wound Care (New Rochelle). 2015. 4(4): 213-224.
[39] W. J. Krause. Krause's Essential Human Histology for Medical Students. 3rd Ed.
USA: Universal Publishers. 2005.
[40] S. Hamid, K. P. Lim, R. B. Zain, S. M. Ismail, S. H. Lau, W. M. Mustafa, et al.
Establishment and characterization of Asian oral cancer cell lines as in vitro
models to study a disease prevalent in Asia. International Journal of Molecular
Medicine. 2007. 19(3): 453-60.
[41] B. Alberts, A. Johnson, J. Lewis, M. Raff, K. Roberts, and P. Walter. Molecular
Biology of the Cell. New York: Garland Science. 2002.
[42] G. M. Cooper. The Cell: A Molecular Approach. 2nd Ed. Sunderland: Sinauer
Associates. 2000.
[43] B. M. Gumbiner. Cell adhesion: the molecular basis of tissue architecture and
morphogenesis. Cell. 1996. 84(3): 345-57.
[44] H. Truong and E. H. Danen. Integrin switching modulates adhesion dynamics
and cell migration. Cell Adhesion & Migration. 2009. 3(2): 179-81.
[45] J. T. Parsons, A. R. Horwitz, and M. A. Schwartz. Cell adhesion: integrating
cytoskeletal dynamics and cellular tension. Nature Reviews Molecular Cell
Biology. 2010. 11(9): 633-43.
[46] K. Burridge, M. Chrzanowska-Wodnicka, and C. Zhong. Focal adhesion
assembly. Trends in Cell Biology. 1997. 7(9): 342-7.
[47] B. Geiger and A. Bershadsky. Assembly and mechanosensory function of focal
contacts. Current Opinion in Cell Biology. 2001. 13(5): 584-92.
[48] R. O. Hynes. Integrins: bidirectional, allosteric signaling machines. Cell. 2002.
110(6): 673-87.
125
[49] C. F. Soon. Development of a novel cell traction force transducer based on
cholesteryl ester liquid crystals. University of Bradford; 2011.
[50] Sigma-Aldrich. Fundamental Techniques in Cell Culture Laboratory Handbook,
2nd ed. vol. 12. 2010.
[51] G. Mazzoleni, D. Di Lorenzo, and N. Steimberg. Modelling tissues in 3D: the
next future of pharmaco-toxicology and food research. Genes & Nutrition. 2009.
4(1): 13-22.
[52] M. W. Tibbitt and K. S. Anseth. Hydrogels as Extracellular Matrix Mimics for
3D Cell Culture. Biotechnology and Bioengineering. 2009. 103(4): 655-663.
[53] K. M. Yamada and E. Cukierman. Modeling tissue morphogenesis and cancer in
3D. Cell 2007. 130: 601-610.
[54] E. Cukierman, R. Pankov, D. R. Stevens, and K. M. Yamada. Taking cell-matrix
adhesions to the third dimension. Science. 2001. 294(5547): 1708-12.
[55] S. K. Muthuswamy. 3D culture reveals a signaling network. Breast Cancer
Research. 2011. 13(1): 103.
[56] L. Kunz-Schughart, J. P. Freyer, F. Hofstaedter, and R. Ebner. The use of 3-D
cultures for high throughput screening: the multicellular spheroid model. Journal
of Biomolecular Screening. 2004. 9(4): 273-285.
[57] C. J. Lovitt, T. B. Shelper, and V. M. Avery. Advanced cell culture techniques
for cancer drug discovery. Biology (Basel). 2014. 3(2): 345-67.
[58] W. Asghar, R. E. Assal, H. Shafiee, S. Pitteri, R. Paulmurugan, and U. Demirci.
Engineering cancer microenvironments for in vitro 3-D tumor models. Materials
Today. 2015. 18(10): 539-553.
[59] M. Ravi, V. Paramesh, S. R. Kaviya, E. Anuradha, and F. D. Solomon. 3D cell
culture systems: advantages and applications. Journal of Cellular Physiology.
2015. 230(1): 16-26.
[60] R. Edmondson, J. J. Broglie, A. F. Adcock, and L. Yang. Three-dimensional cell
culture systems and their applications in drug discovery and cell-based
biosensors. Assay Drug Dev Technol. 2014. 12(4): 207-18.
[61] A. Y. Hsiao, Y. C. Tung, X. Qu, L. R. Patel, K. J. Pienta, and S. Takayama. 384
hanging drop arrays give excellent Z-factors and allow versatile formation of co-
culture spheroids. Biotechnol Bioeng. 2012. 109(5): 1293-304.
126
[62] B. A. Justice, N. A. Badr, and R. A. Felder. 3D cell culture opens new
dimensions in cell-based assays. Drug Discov Today. 2009. 14(1-2): 102-7.
[63] V. Bisceglie. Uber die antineoplastische Immunität; heterologe Einpflanzung von
Tumoren in Hühner-embryonen. Zeitschrift für Krebsforschung. 1933. 40: 122-
140.
[64] T. M. Chang. Semipermeable Microcapsules. Science. 1964. 146(3643): 524-5.
[65] M. Whelehan and I. W. Marison. Microencapsulation using vibrating
technology. Journal of Microencapsulation. 2011. 28: 669-688.
[66] A. Wyss, U. von Stockar, and I. W. Marison. A novel reactive perstraction
system based on liquid-core microcapsules applied to lipase-catalyzed
biotransformations. Biotechnology and Bioengineering. 2006. 93(1): 28-39.
[67] C. Heinzen, A. Berger, and I. Marison. Use of vibration technology for jet break-
up for encapsulation of cells and liquids in monodisperse microcapsules.
Fundamentals of cell immobilisation technology. 2004. 257-275.
[68] R. Atkin, P. Davies, J. Hardy, and B. Vincent. Preparation of aqueous
core/polymer shell microcapsules by internal phase separation. Macromolecules.
2004. 37: 7979-7985.
[69] M. C. Raymond, R. J. Neufeld, and D. Poncelet. Encapsulation of brewers yeast
in chitosan coated carrageenan microspheres by emulsification/thermal gelation.
Artificial Cells Blood Substitutes and Biotechnology. 2004. 32(2): 275-91.
[70] S. Mania. Microcapsules and their applications in pharmaceutical and food
industry. PhD Interdisciplinary Journal. Gdańsk University of Technology; 2013.
[71] D. B. Seifert and J. A. Phillips. Porous alginate--poly(ethylene glycol)
entrapment system for the cultivation of mammalian cells. Biotechnology
Progress. 1997. 13(5): 569-76.
[72] K. A. Heald, T. R. Jay, and R. Downing. Assessment of the reproducibility of
alginate encapsulation of pancreatic islets using the MTT colorimetric assay. Cell
Transplant. 1994. 3(4): 333-7.
[73] S. Wee and W. R. Gombotz. Protein release from alginate matrices. Advanced
Drug Delivery Reviews. 1998. 31(3): 267-285.
[74] E.-S. Chan, B.-B. Lee, P. Ravindra, and D. Poncelet. Prediction models for shape
and size of ca-alginate macrobeads produced through extrusion-dripping method.
Journal of Colloid and Interface Science. 2009. 338: 63-72.
127
[75] M. Whelehan. Microencapsulation by dripping and jet break up.
Bioencapsulation Innovations. 2011.
[76] Y. Zhou, S. i. Kajiyama, H. Masuhara, Y. Hosokawa, T. Kaji, and K. Fukui. A
new size and shape controlling method for producing calcium alginate beads
with immobilized proteins. Journal of Biomedical Science and Engineering.
2009. 2: 287-293.
[77] U. Prube, U. Jahnz, P. Wittlich, J. Breford, and K.-D. Vorlop. Bead production
with JetCutting and rotating disc/nozzle technologies. Landbauforschung
Volkenrode. 2002. 241(1): 1-10.
[78] O. Smidsr d and G. Skja k-Br k. Alginate as immobilization matrix for cells.
Trends in Biotechnology. 1990. 8: 71-78.
[79] T. Sone, E. Nagamori, T. Ikeuchi, A. Mizukami, Y. Takakura, S. Kajiyama, et al.
A novel gene delivery system in plants with calcium alginate micro-beads.
Journal of Bioscience and Bioengineering 2002. 94(1): 87-91.
[80] B. J. Kvam. Conformational conditions and ionic interactions of charged
polysaccharides. Application of NMR techniques and the Poisson-Boltzmann
Equation. Norwegian University of Science and Technology; 1987.
[81] A. Batorsky, J. Liao, A. W. Lund, G. E. Plopper, and J. P. Stegemann.
Encapsulation of adult human mesenchymal stem cells within collagen-agarose
microenvironments. Biotechnol Bioeng. 2005. 92(4): 492-500.
[82] R. R. R. Limin Wang, Jan P. Stegemann. Delivery of Mesenchymal Stem Cells
in Chitosan/Collagen Microbeads for Orthopaedic Tissue Repair. Cells Tissues
Organs. 2013. 197(5): 333-343.
[83] A. Batorsky, J. Liao, A. W. Lund, G. E. Plopper, and J. P. Stegemann.
Encapsulation of adult human mesenchymal stem cells within collagen-agarose
microenvironments. Biotechnology and Bioengineering. 2005. 92(1): 492-500.
[84] V. X. Truong, K. M. Tsang, G. P. Simon, R. L. Boyd, R. A. Evans, H. Thissen,
et al. Photodegradable Gelatin-Based Hydrogels Prepared by Bioorthogonal
Click Chemistry for Cell Encapsulation and Release. Biomacromolecules. 2015.
16(7): 2246-53.
[85] B. Sarker, R. Singh, R. Silva, J. A. Roether, J. Kaschta, R. Detsch, et al.
Evaluation of fibroblasts adhesion and proliferation on alginate-gelatin
crosslinked hydrogel. PLoS One. 2014. 9(9): e107952.
[86] S. N. Tzouanas, A. K. Ekenseair, F. K. Kasper, and A. G. Mikos. Mesenchymal
stem cell and gelatin microparticle encapsulation in thermally and chemically
128
gelling injectable hydrogels for tissue engineering. J Biomed Mater Res A. 2014.
102(5): 1222-30.
[87] S. I. Shinji Sakai, Hitomi Inagaki, Keisuke Hirose, Tomohiro Matsuyama,
Masahito Taya, Koei Kawakami. Cell-enclosing gelatin-based microcapsule
production for tissue engineering using a microfluidic flow-focusing system.
Biomicrofluidics. 2011. 5(013402 ): 1-7.
[88] P. Mercier, F. Fernandez, F. Tortosa, H. Bagheri, H. Duplan, M. Tafani, et al. A
new method for encapsulation of living cells: preliminary results with PC12 cell
line. J Microencapsul. 2001. 18(3): 323-34.
[89] P. S. Clara R. Correia, Rui L. Reisa, João F. Mano. Liquified chitosan–alginate
multilayer capsules incorporating poly(L-lactic acid) microparticles as cell
carriers. Soft Matter. 2013. 9: 2125-2130.
[90] R. K. Ramesh S, Vaikkath D, Nair PD, Madhuri Enhanced encapsulation of
chondrocytes within a chitosan/hyaluronic acid hydrogel: a new technique.
Biotechnol Lett. 2014. 36: 1107-1111.
[91] S. Sakai, K. Kawabata, T. Ono, H. Ijima, and K. Kawakami. Development of
mammalian cell-enclosing subsieve-size agarose capsules (<100 microm) for cell
therapy. Biomaterials. 2005. 26(23): 4786-92.
[92] Uludag H, De Vos P, and T. PA. Technology of mamalian cell encapsulation.
Adv Drug Deliv Rev. 2000. 42(1-2): 29-64.
[93] S. Sugiura, T. Oda, Y. Izumida, Y. Aoyagi, M. Satake, A. Ochiai, et al. Size
control of calcium alginate beads containing living cells using micro-nozzle
array. Biomaterials. 2005. 26(16): 3327-31.
[94] C. Schwinger, S. Koch, U. Jahnz, P. Wittlich, N. G. Rainov, and J. Kressler.
High throughput encapsulation of murine fibroblasts in alginate using the
JetCutter technology. J Microencapsul. 2002. 19(3): 273-80.
[95] P. de Vos, M. M. Faas, B. Strand, and R. Calafiore. Alginate-based
microcapsules for immunoisolation of pancreatic islets. Biomaterials. 2006.
27(32): 5603-17.
[96] P. de Vos, C. G. van Hoogmoed, J. van Zanten, S. Netter, J. H. Strubbe, and H. J.
Busscher. Long-term biocompatibility, chemistry, and function of
microencapsulated pancreatic islets. Biomaterials. 2003. 24(2): 305-12.
[97] S. B. Lucia Picariello, Raffaella Recenti, Lucia Formigli, Alberto Falchetti,
Annamaria Morelli, Laura Masi, Francesco Tonelli, Paolo Cicchi, Maria Luisa
129
Brandi. Microencapsulation of Human Parathyroid Cells: An “in Vitro” Study.
Journal of Surgical Research. 2001. 96: 81-89.
[98] W.-C. P. Min-Hsien Wu Development of microfluidic alginate microbead
generator tunable by pulsed airflow injection for the microencapsulation of cells.
Microfluidics and Nanofluidics. 2010. 8(6): 823-835.
[99] D. R. Irmanida Batubara, Kusdiantoro Mohamad, Wahono Esthi
Prasetyaningtyas. Leydig Cells Encapsulation with Alginate-Chitosan:
Optimization of Microcapsule Formation. Journal of Encapsulation and
Adsorption Sciences. 2012. 2(2): 15-20.
[100] G. S. Moustafa T, Tortosa F, Li R, Sol JC, Rodriguez F, Bastide R, Lazorthes Y,
Sallerin B. Viability and functionality of bovine chromaffin cells encapsulated
into alginate - PLL microcapsules with a liquefied inner core. Cell
Transplantation. 2006. 15(2): 121-133.
[101] P. A.-E. Therese Andersen, Michael Dornish. Review 3D Cell Culture in
Alginate Hydrogels. Microarrays. 2015. 4: 133-161.
[102] S. V. Rocha PM, Gomes ME, Reis RL, Mano JF. Encapsulation of adipose-
derived stem cells and transforming growth factor-beta 1 in carrageenan-based
hydrogels for cartilage tissue engineering. J. Bioactive Compatible Polym. 2011.
26: 493-507.
[103] H. S. Rokstad AM, Strand B, Steinkjer B, Ryan L, Kulseng B, Skjåk-Braek G,
Espevik T. Microencapsulation of cells producing therapeutic proteins:
optimizing cell growth and secretion. Cell Transplantation. 2002. 11(4): 313-
324.
[104] D. S. AYYILDIZ, Mert; ELİBOL, Murat; GüRHAN, S. İsmet DELİLOĞU.
Cultivation of Calcium-Alginate Encapsulated Myeloma Cells in a Bioreactor.
International Journal of Natural & Engineering Sciences. 2009. 3(2): 48-53.
[105] P. B. Lee GM. Stability of antibody productivity is improved when hybridoma
cells are entrapped in calcium alginate beads. Biotechnol Bioeng. 1993. 42(9):
1131-1135.
[106] B. C. C. Martin S. Sinacore, Robert Buehler. Entrapment and Growth of Murine
Hybridoma Cells in Calcium Alginate Gel Microbeads. Nature Biotechnology.
1989. 7: 1275-1279.
[107] J. M. S. S. Overgaard, M. Moo-Young, N. C. Bols. Immobilization of hybridoma
cells in chitosan alginate beads. The Canadian Journal of Chemical Engineering.
1991. 69(2): 439-443.
130
[108] H. J. Plunkett ML. An in vivo quantitative angiogenesis model using tumor cells
entrapped in alginate. Lab Invest. 1990. 62(4): 510-517.
[109] Q. C. Yong Wang, Fan Yuan. Alginate encapsulation is a highly reproducible
method for tumor cell implantation in dorsal skinfold chambers. BioTechniques.
2005. 39: 834-839.
[110] R. G. Veronique Breguet, Urs von Stockar, Ian William Marison. CHO
immobilization in alginate/poly-l-lysine microcapsules: an understanding of
potential and limitations. Cytotechnology. 2007. 53(1-3): 81-93.
[111] C.-H. W. Jingwei Xiea. Electrospray in the dripping mode for cell
microencapsulation. Journal of Colloid and Interface Science. 2007. 312(2):
247-255.
[112] A. D. Suttiruk Jitraruch, Robin D. Hughes, Celine Filippi, Daniel and C. P.
Soong, Sharon C. Lehec, Nigel D. Heaton, Maria S. Longhi, Ragai R. Mitry.
Alginate Microencapsulated Hepatocytes Optimised for Transplantation in Acute
Liver Failure. PLoS ONE. 2014. 9(12): e113609 (1-23).
[113] L. D.-S. Um E, Pyo H-B, Park J-K. Continuous generation of hydrogel beads and
encapsulation of biological materials using a microfluidic droplet merging
channel. Microfluid Nanofluid. 2008. 5: 541-549.
[114] K. S. L. Choong Kim, Young Eun Kim, Kyu-Jung Lee, Soo Hyun Lee, Tae Song
Kima, Ji Yoon Kang. Rapid exchange of oil-phase in microencapsulation chip to
enhance cell viability. Lab Chip. 2009. 9: 1294-1297.
[115] R. Barer. Some Applications of Phase-contrast Microscopy. Quarterly Journal of
Microscopical Science. 1947. 3: 491-499.
[116] O. Debeir, P. Van Ham, R. Kiss, and C. Decaestecker. Tracking of migrating
cells under phase-contrast video microscopy with combined mean-shift
processes. IEEE Transactions on Medical Imaging. 2005. 24(6): 697-711.
[117] R. Barer. Some Applications of Phase-contrast Microscopy. Quarterly Journal of
Microscopical Science. 1947. 3: 491-499.
[118] D. B. Murphy and M. W. Davidson. Fundamentals of Light Microscopy and
Electronic Imaging: Wiley-Blackwell. 2012.
[119] D. G. Dalgleish, P. A. Spagnuolo, and H. D. Goff. A possible structure of the
casein micelle based on high-resolution field-emission scanning electron
microscopy. International Dairy Journal. 2004. 14(12): 1025-1031.
131
[120] Y. Yuan, Y. Shimada, S. Ichinose, and J. Tagami. Qualitative analysis of
adhesive interface nanoleakage using FE-SEM/EDS. Dental Materials. 2007.
23(5): 561-9.
[121] H. J. Gulley-Stahl, J. A. Haas, K. A. Schmidt, A. P. Evan, and A. J. Sommer.
Attenuated Total Internal Reflectance Infrared Spectroscopy (ATR-FTIR): A
Quantitative Approach for Kidney Stone Analysis. Applied Spectroscopy. 2009.
63(7): 759-766.
[122] N. Puviarasan, V. Arjunan, and S. Mohan. FT-IR and FT-Raman Studies on 3-
Aminophthalhydrazide and N-Aminophthalimide. Turkish Journal of Chemistry.
2002. 26: 323-333.
[123] M. Deneva. Infrared spectroscopy investigation of metallic nanoparticles based
on copper, cobalt, and nickel synthesized through borohydride reduction method
(review). Journal of Chemical Technology and Metallurgy. 2010. 45(4): 351-
378.
[124] A. Krishan and P. D. Dandekar. DAPI fluorescence in nuclei isolated from
tumors. Journal of Histochemistry & Cytochemistry. 2005. 53(8): 1033-6.
[125] J. Kapuscinski. DAPI: a DNA-specific fluorescent probe. Biotechnic &
Histochemistry. 1995. 70(5): 220-33.
[126] J. Portugal, and M. J. Waring. Assignment of DNA binding sites for 4', 6-
diamidine-2-phenylindole and bisbenzimide (Hoechst 33258). A comparative
footprinting study. Biochimica et Biophysica Acta. 1988. 949(2): 158-168.
[127] I. Johnson, and M. Spence. Molecular Probes Handbook. A guide to fluorescent
probes and labeling technologies. 11th Ed. United States: Life Technologies.
2010.
[128] H. L. Bara. Tissue Engineering a Pancreatic Substitute Based on Recombinant
Intestinal Endocrine Cells. Ph.D. Thesis. Emory University; 2008.
[129] C. F. Soon, W. I. Omar, R. F. Berends, N. Nayan, H. Basri, K. S. Tee, et al.
Biophysical characteristics of cells cultured on cholesteryl ester liquid crystals.
Micron. 2014. 56: 73-9.
[130] H. A. Crissman and G. T. Hirons. Staining of DNA in live and fixed cells.
Methods in Cell Biology. 1994. 41: 195-209.
[131] S. Sakai, S. Ito, Y. Ogushi, I. Hashimoto, N. Hosoda, Y. Sawae, et al.
Enzymatically fabricated and degradable microcapsules for production of
multicellular spheroids with well-defined diameters of less than 150 microm.
Biomaterials. 2009. 30(30): 5937-42.
132
[132] Q. Gao, Y. He, J.-z. Fu, J.-j. Qiu, and Y.-a. Jin. Fabrication of shape controllable
alginate microparticles based on drop-on-demand jetting. Journal of Sol-Gel
Science and Technology. 2016. 77(3): 610-619.
[133] S. Haeberle, L. Naegele, R. Burger, F. von Stetten, R. Zengerle, and J. Ducree.
Alginate bead fabrication and encapsulation of living cells under centrifugally
induced artificial gravity conditions. J Microencapsul. 2008. 25(4): 267-74.
[134] S. V. Bhujbal, B. de Haan, S. P. Niclou, and P. de Vos. A novel multilayer
immunoisolating encapsulation system overcoming protrusion of cells. Scientific
Reports. 2014. 4: 6856.
[135] K. Kevekordes. Using light scattering measurements to study the effects of
monovalent and divalent cations on alginate aggregates. Journal of Experimental
Botany. 1996. 47(298): 677-682.
[136] T. A. B. Bressel, A. H. Paz, G. Baldo, E. O. C. Lima, U. Matte, and M. L.
Saraiva-Pereira. An effective device for generating alginate microcapsules.
Genetics and Molecular Biology. 2008. 31(1): 136-140.
[137] H. Daemi and M. Barikani. Synthesis and characterization of calcium alginate
nanoparticles, sodium homopolymannuronate salt and its calcium nanoparticles.
Scientia Iranica F. 2012. 19(6): 2023-2028.
[138] A. D. Meade, H. J. Byrne, and F. M. Lyng. Spectroscopic and chemometric
approaches to radiobiological analyses. Mutation Research. 2010. 704(1-3): 108-
14.
[139] A. D. Meade, C. Clarke, H. J. Byrne, and F. M. Lyng. Fourier transform infrared
microspectroscopy and multivariate methods for radiobiological dosimetry.
Radiation Research. 2010. 173(2): 225-37.
[140] A. D. Meade, F. M. Lyng, P. Knief, and H. J. Byrne. Growth substrate induced
functional changes elucidated by FTIR and Raman spectroscopy in in-vitro
cultured human keratinocytes. Analytical and Bioanalytical Chemistry. 2007.
387(5): 1717-28.
[141] M. Nagpal, S. K. Singh, and D. Mishra. Synthesis characterization and in vitro
drug release from acrylamide and sodium alginate based superporous hydrogel
devices. International Journal of Pharmaceutical Investigation. 2013. 3(3): 131-
40.
[142] Polona Smrdel, Marija Bogataj, and A. Mrhar. The influence of selected
parameters on the size and shape of alginate beads prepared by ionotropic
gelation. Journal of Pharmaceutical Sciences. 2008. 76: 77-89.
133
[143] D. Kabelitz and S. H. E. Kaufmann. Immunology of Infection. vol. 37, ed UK:
Academic Press, pp. 145-146; 2010.
[144] J. W. Haycock. 3D cell culture: a review of current approaches and techniques.
Methods in Molecular Biology. 2011. 695: 1-15.
[145] Y. R. Lou, L. Kanninen, B. Kaehr, J. L. Townson, J. Niklander, R. Harjumaki, et
al. Silica bioreplication preserves three-dimensional spheroid structures of
human pluripotent stem cells and HepG2 cells. Scientific Reports. 2015. 5:
13635.
[146] R. J. DeBerardinis, J. J. Lum, G. Hatzivassiliou, and C. B. Thompson. The
biology of cancer: metabolic reprogramming fuels cell growth and proliferation.
Cell Metabolism. 2008. 7(1): 11-20.
[147] T. Yeung, P. C. Georges, L. A. Flanagan, B. Marg, M. Ortiz, M. Funaki, et al.
Effects of substrate stiffness on cell morphology, cytoskeletal structure, and
adhesion. Cell Motility and the Cytoskeleton. 2005. 60(1): 24-34.