biocompatible smart microcapsules based on chitosan-poly(vinyl alcohol) copolymers for cultivation...
TRANSCRIPT
RE
DOI: 10.1002/adem.201180014SEARCH
ART
Biocompatible Smart Microcapsules Based onChitosan-Poly(vinyl alcohol) Copolymers for Cultivation ofAnimal Cells**
ICLE
By Daria Zaytseva-Zotova, Vera Balysheva, Anna Tsoy, Maria Drozdova,Tatiana Akopova, Leonid Vladimirov, Isabelle Chevalot, Annie Marc,Jean-Louis Goergen and Elena Markvicheva*
In this study, two novel chitosan-graft-poly(vinyl alcohol) copolymers are synthesized and used aswater-soluble at physiological conditions polycations for preparation of smart microcapsules. Themicrocapsules provide growth and proliferation of eight mammalian cell lines, including hybridomaand tumor cells, at long-term cell cultivation in vitro. The microcapsules are stable in cell culturemedium but can be dissolved by changing pH value of the medium (up to 8.0–8.2), thus making possiblea simple release of the entrapped cells. Monoclonal antibody production by encapsulated hybridomacells is demonstrated. Cultivation of tumor cells within the microcapsules allows the formation of 3Dmulticellular spheroids, which can be proposed as an in vitro model for anticancer drug screening.
Presently cell microencapsulation is widely employed in
biomedicine and biotechnology.[1] Biocompatible polymer
microcapsules for animal cell entrapment were proposed by F.
Lim and A. M. Sun in the beginning of the 1980 s.[2] To form
semipermeable polyelectrolyte membranes of the microcap-
sules, they chose natural polysaccharide alginate (polyanion)
and positively charged synthetic polypeptides (polycations),
for instance poly(L-lysine) (PLL), poly(L-arginine), poly(-
L-ornithin), etc.
[*] Prof. E. Markvicheva, D. Zaytseva-Zotova, A. TsoyM. DrozdovaPolymers for Biology Laboratory, Shemyakin & OvchinnikovInstitute of Bioorganic Chemistry of Russian Academy of Sciences,Miklukho-Maklaya str., 16/10, Moscow, 117997, (Russia)E-mail: [email protected]
Prof. V. BalyshevaAll-Russian Research Institute for Veterinary Virology andMicrobiology, Russian Academy of Agricultural Sciences,Pokrov, Vladimir region 601120, (Russia)
Dr. T. Akopova, Prof. L. VladimirovN.S. Enikolopov Institute of Synthetic Polymer Materials,Russian Academy of Sciences, Profsouznaya str., 70, Moscow117393, (Russia)
Prof. I. Chevalot, Prof. A. Marc, Prof. J.-L. GoergenLaboratoire Reactions et Genie des Procedes, UPR CNRS3349, ENSAIA-INPL, 2, Avenue de la Foret de Haye, BP 172,Vandoeuvre-les-Nancy, 54505, (France)
ADVANCED ENGINEERING MATERIALS 2011, 13, No. XX � 2011 WILEY-VCH
It is well known today that the polyelectrolyte micro-
capsules provide a free exchange of nutrients, gases (O2 and
CO2), and a release of metabolites and cell products through
semipermeable polymer membrane of the microcapsule.[3]
Being implanted into the body, microcapsules can play a dual
role: they can work as microreactors providing release of
therapeutics (recombinant proteins and peptides) secreted by
cells through the membranes, and at the same time they can
protect the encapsulated cells against patient immune cells.[4]
[**] This work was partially supported by the bilateral Russian-French program (the joint CNRS-RFBR PICS project N.10-04-91056) and also by RFBR project N. 10-03-01022.The authors are grateful to Dr. J. McGuire (Roswell ParkCancer Institute, Buffalo, USA) for the kind gift of humanleukemia cell lines and to Dr. T. Erokhina (Shemyakin &Ovchinnikov Institute of Bioorganic Chemistry of RAS, Russia)for mouse myeloma Sp2/0 cells. The authors are also thankful toProf. E. Vodovozova (Shemyakin & Ovchinnikov Institute ofBioorganic Chemistry of RAS, Russia) and to Prof. A. Bartko-wiak (Westpomeranian University of Technology, Poland) fortheir kind support of this research.
Verlag GmbH & Co. KGaA, Weinheim wileyonlinelibrary.com B1
RESEARCH
ARTIC
LE
D. Zaytseva-Zotova et al./Biocompatible Smart Microcapsules Based on Chitosan-Poly(vinyl alcohol) . . .
The main advantages of microencapsulation as a three-
dimensional (3D) growth technique are chemically and
spatially defined 3D network of extracellular matrix compo-
nents, cell-to-cell and cell-to-matrix interactions which govern
differentiation, proliferation, and cell function in vivo. These,
in fact, are lost under the simplified two-dimensional (2D)
conditions.[5]
All the mentioned issues allow to consider microencapsu-
lation as a promising technique for a number of biomedical
applications, including diabetes treatment,[6] somatic gene
therapy,[7] tissue engineering,[8] and anticancer drug screen-
ing using microencapsulated multicellular tumor spheroids
(MTS).[9]
Cell microencapsulation was widely used to support
growth of cells, such as insulin-producing pancreatic
beta-cells (Langerhans islets),[10] parathyroid cells,[11] hepa-
tocytes,[12] stem cells,[13] and hybridoma cells.[14]
Howbeit, cell microencapsulation technique requires an
improvement of procedures, materials, and devices for
microcapsule preparation.[15] Chitosan-based polymers seem
to be a good alternative to replace commonly used PLL or
other rather expensive polypeptides, since natural poly-
saccharides (e.g., chitosans) are cheaper. Moreover, a direct
comparison showed that the toxic effect of alginate-PLL
membrane was significantly higher than those for chito-
sans.[16] However, as well known, high molecular weight
chitosans are soluble only at acidic pH value while cell
encapsulation procedure should be carried out under
physiological conditions (pH 6.8–7.2). The grafting of
chitosans with biocompatible water-soluble synthetic poly-
mers, e.g., poly(vinyl alcohol) (PVA), could be a promising
approach. Unlike chitosans, such copolymers can be soluble at
neutral pH and seem to be promising for animal cell
encapsulation.
Thus, the aim of the current research was to fabricate
biocompatible smart microcapsules based on a novel
chitosan-g-PVA copolymers and to demonstrate capability
of these microcapsules to support growth of various
mammalian cells at long-term cultivation in vitro.
Results and Discussion
Chitosan-Based Polycations
Chitosans belong to a family of natural biocompatible
cationic pH-sensitive polysaccharides produced by partial
deacetylation of chitin from reprocessing of seafood waste.
However, high molecular weight chitosans are soluble at
acidic pH values, and therefore, cannot be used for animal cell
encapsulation while oligochitosans (Mw¼ 3.0–10.0 kDa) are of
great interest, since they are soluble at physiological pH.[17]
Moreover, oligochitosans have been recently reported for
preparation of microcapsules to entrap cells.[9]
On the other hand, PVA is a biocompatible water-
soluble synthetic polymer widely employed for biomedical
applications, e.g., for controlled drug delivery and tissue
engineering.[18]
B2 http://www.aem-journal.com � 2011 WILEY-VCH Verlag GmbH & Co
To combine the desirable properties of chitosan and
PVA, in particular, chitosan pH-sensitivity and PVA
water solubility at physiological conditions (pH 7.2), we
synthesized PVA-g-chitosan copolymers. These copolymers
were prepared by a novel solid-state reactive blending (SSRB)
method.
The uniqueness of this method relies upon a variety of
chemical (e.g., grafting, polymer-analogous transformation,
polymerization, and polycondensation reactions) and physi-
cal transformations of solid polymers and monomers which
occurred at joint action of high pressure and shear deforma-
tion. The method is based on the reactive blending of all
compounds at plastic flow conditions by applying an external
mechanical energy to polymeric solid mixtures. Currently,
organic reactions that occur under these conditions, so called
‘‘solvent-free reactions,’’ are of great interest. These reactions
have numerous advantages over common reactions in
solution, since they are infinitely high concentration reactions.
Furthermore, in many cases they proceed faster, more
selectively, and much more efficiently compared to solution
reactions.[19] Treatment of polymers under these conditions
results in substantial changes of their structure, viz. crystal-
linity, degree of particle dispersability, reactivity of the
functional groups in heterogeneous reactions, etc.[20]
Thus, this novel technique seems to be promising to modify
infusible and poorly soluble polymers substances like
polysaccharides (e.g., chitin).[21] For example, chitosan (with
�100% yield) can be produced by alkaline solid-state
deacetylation of chitin in the extruder.[22]
In our work, two chitosan-g-PVA copolymers were
prepared by SSRB method using a coextrusion of chitin with
PVAc in the presence of sodium hydroxide. FTIR spectro-
scopy analysis showed that deacetylation degree of both
copolymers was almost complete (up to 95–98%). It was also
revealed that the polymer-analogous transformations under
these conditions were accompanied by a formation of an
extensively grafted copolymeric system. Water-soluble at
room temperature fractions of the obtained products (� 20%
of entire systems) were characterized. Both FTIR and
elemental analyses were used to evaluate the chitosan content
in the obtained fractions. FTIR spectra of the samples after
copolymer purification and precipitation from aqueous
solutions contained characteristic absorption PVA and
chitosan bands (Fig. 1 and 2). Figure 1 shows FTIR spectra
for chitosan-g-PVA1 copolymer (curve 1) and chitosan (curve
2). As can be seen in Figure 1 copolymer spectrum contains the
band of OH stretching (3 400 cm�1) along with the presence of
CH2� bending at 850 cm�1. Figure 2 demonstrates FTIR
spectrum for chitosan-g-PVA20 sample (curve 2) compared to
a model chitosan/PVA (20:80 w/w) mixture (curve 1). The
calculations showed that the chitosan contents in the obtained
copolymers were 80 and 15 wt% for chitosan-g-PVA1 and
chitosan-g-PVA20, respectively. Glucosamine contents for
chitosan and both copolymers were also calculated from
the results of elemental analysis using C/N ratio (5.29 in
the case of initial chitosan). Elemental analysis data for
. KGaA, Weinheim ADVANCED ENGINEERING MATERIALS 2011, 13, No. XX
RESEARCH
ARTIC
LE
D. Zaytseva-Zotova et al./Biocompatible Smart Microcapsules Based on Chitosan-Poly(vinyl alcohol) . . .
Fig. 1. FTIR spectra of chitosan-g-PVA1 copolymer (curve 1) and chitosan (curve 2).Chitosan-g-PVA1 copolymer contains 80 wt% of chitosan.
Fig. 2. FTIR spectra of the chitosan/PVA (20:80 w/w) model mixture (curve 1) and thechitosan-g-PVA20 (15 wt% of chitosan) copolymer (curve 2).
chitosan-g-PVA1 sample are (found/calculated, %): C, 46.83/
46.69; N, 6.83/6.94; O, 39.02/39.07; H, 7.32/7.28; for
chitosan-g-PVA20 sample: C, 52.96/53.05; N, 1.40/1.32; O,
36.91/36.87; H, 8.73/8.74. Calculations from the results of
elemental analysis using C/N ratio for both pure chitosan and
chitosan-g-PVA copolymers were in a good agreement with
FTIR data. It was also revealed that the chitosan content in the
prepared copolymers was a function of PVAc/chitin molar
ratio in the initial mixtures. The increase of PVAc content in
the initial reactive mixture resulted in the decrease of chitosan
content in the obtained copolymer. Thus, in the case of
chitosan-g-PVA1 sample PVA/chitosan molar ratio was 0.92
when the initial PVAc/chitin ratio was 1.4. It was increased up
to 20.5 (in the chitosan-g-PVA20 sample) when the initial
PVAc/chitin ratio was enhanced up to 3. It could be suggested
that PVA in chitosan-g-PVA1 copolymer was statistically
distributed in the form of relatively short chains grafted onto
chitosan. This result is in a good agreement with a theory of
mechano-induced destruction of polymer chains. We suppose
that PVAc as a component with a flexible chain can act as a
surfactant, thus providing an increase in plasticity of the
ADVANCED ENGINEERING MATERIALS 2011, 13, No. XX � 2011 WILEY-VCH Ve
systems under coextrusion. The values of Mw of the obtained
copolymers determined by GPC method were 124 and
190 kDa for chitosan-g-PVA1 and chitosan-g-PVA20 samples,
respectively. Both obtained chitosan-g-PVA copolymers were
water-soluble at physiological conditions (pH 7.2, room
temperature).
Microcapsules
To form stable microcapsules of the desired size and
polyelectrolyte membrane thickness, alginate (polyanion)
and two chitosan-g-PVA copolymers or oligochitosan (poly-
cations) were used. The microcapsules were prepared in three
steps: (1) a dropwise addition of a NaAlg solution with
suspended cells to a CaCl2 solution to get CaAlg microbeads;
(2) an incubation of the obtained CaAlg microbeads in a
polycation solution to form a polyelectrolyte membrane on the
CaAlg microbead surface; (3) a treatment of the obtained
microbeads with a chelating agent solution (EDTA), in order
to dissolve the alginate core and to get hollow microcapsules.
The microcapsule shape, diameter, and size distribution
depended on initial characteristics of CaAlg microbeads.
Usually, various dispersion techniques for fabrication of
microbeads with the diameters ranged from 150 to 900 mm are
employed. In this study a special device with a coaxial air flow
was used. It allowed to break the NaAlg solution flow thus
decreasing the NaAlg drop size just on a needle tip before the
drops fell into the CaCl2 solution. Optimal conditions for the
preparation of CaAlg microbeads by this technique were
described earlier.[9] Here, the mean diameter of the obtained
microbeads was 750� 50 mm.
On the next step, microcapsules were formed by incubation
of the CaAlg microbeads in the polycation solution. The
thickness of the microcapsule membrane depended upon the
polycation type, concentration of the polycation solution, and
the incubation time (Table 1). If the incubation time was not
long enough for membrane formation, the microcapsules were
completely dissolved at the EDTA solution treatment. On the
other hand, when the incubation time was too long, the CaAlg
microbeads were fully cross-linked by the polycation, and the
microcapsule membrane was not observed under a light
microscope. As a result of optimization, mechanically stable
microcapsules with an optimal membrane thickness were
obtained after the CaAlg beads incubation in oligochitosan,
chitosan-g-PVA1, and chitosan-g-PVA20 solutions for 5, 5, and
10 min, respectively.
The obtained microcapsules had a larger diameter
than the appropriate CaAlg microbeads, and their swelling
behavior in the physiological solution depended on the
type of the polycation we used (Table 1). This can be explained
by the difference in Mw and the polycation type. More was the
content of hydrophilic PVA in the chitosan-g-PVA copolymer,
higher swelling of the microcapsules was observed.
Nevertheless, all the microcapsules withstand centrifuga-
tion (9 000� g) for 10 min. The obtained microcapsules had a
nice spherical shape and were stable in both physiological
rlag GmbH & Co. KGaA, Weinheim http://www.aem-journal.com B3
RESEARCH
ARTIC
LE
D. Zaytseva-Zotova et al./Biocompatible Smart Microcapsules Based on Chitosan-Poly(vinyl alcohol) . . .
Table 1. Membrane thickness of microcapsules in function of polycation type and incubation time.
Polycation sample Microcapsule meandiameter [mm]
Polycation solutionconcentration [%]
Membrane thickness as functionof incubation time [mm]
5 [min] 7 [min] 10 [min]
Oligochitosan 900� 75 0.10 78� 5 112� 6 n.d.[a]
0.20 89� 5 135� 6 n.d.
Chitosan-g-PVA1[b] 780� 50 0.20 27� 5 – 54� 5
0.25 51� 5 76� 5 n.d.
0.50 81� 5 – n.d.
Chitosan-g-PVA20[c] 1150� 80 0.75 – 37� 5 66� 5
1.15 – 42� 5 87� 5
[a] Membrane was not detected;
[b] Chitosan/PVA ratio was 80:20w/w,Mw¼ 124 kDa;
[c] Chitosan/PVA ratio was 15:85 w/w,Mw¼ 190 kDa.
Table 2. The list of cell lines grown in alginate-polycation microcapsules.
Cell line Oligochitosan Chitosan-g-PVA1 Chitosan-g-PVA20 Cell line characteristics:origin/growth properties
Time needed to fillmicrocapsule volume [days]
CCRF-CEM n.d.[a] þ þ Human/suspension 18
CEM/C1 n.d. þ þ Human/suspension 22
1D2 þ n.d. n.d. Mouse/suspension 11
Sp2/0 (Ag14) þ[b] þ n.d. Mouse/suspension 14
P388D1 þ n.d. þ Mouse/suspension 28
MCF-7 þ n.d. n.d. Human/adherent 28
M-3 �[c] – – Mouse/adherent –
BHK-21 þ n.d. n.d. Hamster/adherent 11
PSGK-60 þ n.d. n.d. Siberian mountain goat/adherent 14
[a] n.d., not determined;
[b] ‘‘þ ’’ Cell aggregates formed within the microcapsules;
[c] ‘‘� ’’ Cell aggregates did not form within microcapsules.
solution and in the cultivation medium for 4 weeks. Therefore,
we suggested that the obtained microcapsules with the
optimal membrane thickness of 80–100 mm could be used for
long-term cell cultivation.
Since the chitosan-g-PVA copolymers were pH-sensitive
due to chitosan, the microcapsules were shown to be easily
dissolved by slightly increasing pH value of the incubation
medium. For instance, the replacement of the physiological
solution for a culture medium with increased pH (8.0–8.2)
resulted in membrane dissolving.
Thus, the use of novel chitosan-g-PVA polycations makes
possible simple cell release from the microcapsules after
long-term cell cultivation by slight increasing pH of cultiva-
tion medium up to 8.0–8.2, if further manipulations with the
obtained multicellular spheroids are needed.
Growth of Cells in Microcapsules
In order to test three types of microcapsules for their
capability to support cell growth, various cells differed in their
origin (human, mouse, etc.), and growth properties (suspen-
sion culture or monolayer) were chosen for microencapsula-
tion. The optimal initial cell concentration used for micro-
B4 http://www.aem-journal.com � 2011 WILEY-VCH Verlag GmbH & Co
encapsulation was found to be (1.0� 0.2)� 106 cells �mL�1of
the NaAlg solution. This concentration allowed to form
microcapsules with rather homogeneous cell distribution
inside them (70–150 cells per microcapsule).
Table 2 demonstrates the ability of various cell lines to grow
within the microcapsules. This ability depended upon cell
line properties but did not depend strongly on the polycation
type we used. Thus, we got multicellular spheroids within the
microcapsules for almost all selected cell lines, except M3
mouse melanoma cells. Melanoma cells grew on the inner
microcapsule membrane but did not fill the microcapsule
volume, since their growth most probably was suppressed,
although there was a lot of space inside the microcapsule.
Thus, eight different cell lines were successfully cultivated
within the microcapsules for 2–4 weeks. Typical growth
dynamics for encapsulated cells is presented in Figure 3.
Initially myeloma Sp2/0 cells distributed evenly as single cells
within the microcapsules. After being cultured for 5 d, the
cells formed small aggregates. These aggregates increased in
their sizes and filled the whole microcapsule volume in 14 d
after microencapsulation. As can be seen, the cell growth
did not depend on polycation type chosen for membrane
formation.
. KGaA, Weinheim ADVANCED ENGINEERING MATERIALS 2011, 13, No. XX
RESEARCH
ARTIC
LE
D. Zaytseva-Zotova et al./Biocompatible Smart Microcapsules Based on Chitosan-Poly(vinyl alcohol) . . .
Fig. 3. Myeloma Sp2/0 cell growth in alginate/oligochitosan (A–D) and alginate/chitosan-g-PVA1 (E–H) microcapsules at day 1 (A and E), day 5 (B and F), day 10 (C and G), andday 14 (D and H). The microcapsule membrane is indicated with arrows. Scale bar is 300 mm.
Fig. 4. Growth kinetics of 1D2 hybridoma cells and BHK-21 cells in the microcapsules.
Fig. 5. Titers of MAbs produced by encapsulated 1D2 hybridoma cells in the cultivationmedium. Arrows indicate the time when the culture medium was completely replaced.
Figure 4 shows the growth kinetics of microencapsulated
BHK-21 cells and 1D2 hybridoma cells for 21 d of cultivation.
Cell concentration increased 10-fold within first 5 d,
and it reached the values of 7� 106 cells �mL�1 and
4.5� 106 cells �mL�1 for BHK-21 and 1D2 cells, respectively,
by day 11th. On day 11 alive cell concentration decreased while
dead cell concentration raised. This could be explained by high
cell density within the microcapsules resulting in the decrease
of nutrients diffusion and limitation of oxygen supply.
Thus, the developed microcapsules were capable to
provide growth of eight cell lines at long-term cultivation
up to 1 month.
Production of Monoclonal Antibodies (MAbs) by EncapsulatedCells
As well known, cell microencapsulation provides a number
of technical advantages for a large-scale MAbs production as
well as it allows a sustained and controlled delivery of the de
novo produced therapeutic product. Moreover, cell entrap-
ment in microcapsules with semipermeable membranes could
ADVANCED ENGINEERING MATERIALS 2011, 13, No. XX � 2011 WILEY-VCH Ve
be used to reduce or in some cases even to avoid chronic
administration of immunosuppressive drugs.[14]
In the current study 1D2 hybridoma cells producing MAbs
against IgG heavy chain were chosen as a model cell line. The
samples of the culture medium were collected daily and
concentration of MAbs released from microcapsules was
determined by enzyme-linked immunosorbent assay (ELISA;
Fig. 5). Suspension cell culture was used as a control. Cells
entrapped in the microcapsules presented rather higher MAbs
production after first 9 d. The total volume of the medium
containing MAbs was 800 mL within 21 d. These results
confirmed that the developed microcapsules could be used for
MAbs production by entrapped cells.
Generation of Multicellular Tumor Spheroids in Microcapsules
Cell microencapsulation is a promising approach to
develop a novel in vitro 3D model, which could rather well
mimic small size solid tumors. R. M. Sutherland was the first
to propose MTS as a more adequate model of small solid
rlag GmbH & Co. KGaA, Weinheim http://www.aem-journal.com B5
RESEARCH
ARTIC
LE
D. Zaytseva-Zotova et al./Biocompatible Smart Microcapsules Based on Chitosan-Poly(vinyl alcohol) . . .
Fig. 6. MCF-7 cell viability in encapsulated MTS and in a monolayer culture as afunction of MTX concentration.
tumors compared to 2D suspension or monolayer cultures.[23]
MTS have been demonstrated to represent quite properly
the 3D growth and organization of solid tumors, and
consequently to better mimic cell–cell interactions and
microenvironment in a tumor tissue.[24] Due to these
similarities to a tumor xenograft, MTS have become a
valuable tool in tumor biology. Nowadays, MTS are widely
used as an in vitro model for various biomedical studies
related to cancer therapy, e.g., radiotherapy or photodynamic
therapy.[25] A classical technique for MTS formation
includes cultivation of anchorage-dependent cells at stirring
which prevents cell attachment to a surface and results in
cell growing as aggregates finally forming multicellular
spheroids.
Although many techniques are presently available to get
3D tissue models in vitro,[26] all of them have inherent
limitations. Thus, commonly used in vitro classical methods,
such as liquid-overlay, spinner flask and gyratory rotation
systems are time consuming and cannot provide production
of MTS with narrow spheroid size distribution within a
desired range. These disadvantages can be easily overcome
using microencapsulation for MTS generation. The approach
based on tumor cell encapsulation as a novel technique to
quickly and easily prepare a large number of microencapsu-
lated MTS with narrow size distribution within a desired
diameter has been reported by us quite recently.[9]
In the present study microencapsulated MTS were
obtained for four various tumor cell lines (e.g., human cell
lines CCRF-CEM, CEM/C1, MCF-7, and mouse Sp2/0 cells).
As can be seen in Figure 3, Sp2/0 cells formed a compact
multicellular clusters within the microcapsules at long-term
cultivation already on day 14.
Adenocarcinoma MCF-7 cells was chosen as a model cell
line to demonstrate that the encapsulated MTS could be
considered as a more rapid and valid in vitro model compared
to a monolayer culture for evaluation of anticancer drugs.
The MTX cytotoxicity was estimated as an inhibition rate
in cell viability. To evaluate non-specific sorption of MTX by
the microcapsules, cell viability in the monolayer culture
sample containing empty microcapsules was tested. It was
found that non-specific MTX sorption by the microcapsules
was insignificant (3–5%). The cell viability decreased with
increasing drug concentration in both encapsulated MTS
and the monolayer culture (Fig. 6). However, the inhibition
rate in encapsulated MTS was much lower than that for the
monolayer culture. Thus, the IC50 (a half maximal inhibitory
concentration) was 55 and 2.7� 10�9M for MTS and
monolayer, respectively. These results demonstrated that
microencapsulated MTS were more resistant to anticancer
drug treatment than the monolayer culture.
Conclusions
Chitosan-g-PVA copolymers were obtained by a novel
SSRB method. Biocompatible smart microcapsules based on
the polyelectrolyte complex between alginate and chitosan-
B6 http://www.aem-journal.com � 2011 WILEY-VCH Verlag GmbH & Co
based polycations (oligochitosan or chitosan-g-PVA copoly-
mers) were elaborated. The microcapsules fabricated from
alginate and chitosan-g-PVA copolymers were stable during
long-term cell cultivation. Multicellular spheroids generated
within these microcapsules could be easily released by slightly
rising pH value of the culture medium up to pH 8.0–8.2, since
the microcapsules were pH-sensitive. The novel polyelec-
trolyte microcapsules were demonstrated to support growth
and proliferation of eight animal cell lines differed in their
growth properties and origin. Our results also indicated that
the microcapsules could be successfully used for production
of MAbs by 1D2 hybridoma cells at their long-term cultivation
for 21 d. Moreover, encapsulated tumor cells were able to
generate multicellular spheroids, which could be used as an in
vitro model to test chemotherapeutic drugs, namely MTX.
Thus, the developed biocompatible smart microcapsules
embedded with different animal cells could be proposed
for several biomedical applications.
Experimental
Chemicals
Alginic acid sodium salt (NaAlg; medium viscosity, approx.
3 500 cps at 25 8C), EDTA sodium salt, bovine serum albumin (BSA),
mouse IgG antibodies, horseradish peroxidase-linked goat anti-rat
IgG conjugate, and methotrexate (MTX) were from Sigma–Aldrich
(Germany). Calcium chloride (CaCl2� 2H2O) was purchased from
Panreac (Spain). PBS (pH 7.2), Tween-20, sodium chloride (NaCl),
and Trypan Blue were from PanEco (Russia), Serva (Germany),
REACHEM (Russia), and FlowLaboratories (Germany), respec-
tively.
Oligochitosan (Mw¼ 3.5 kDa, deacetylation degree 89%) was
kindly provided by Prof. A. Bartkowiak (Poland). For synthesis of
chitosan-g-PVA copolymers, a-chitin (Mw¼ 650 kDa) isolated from
crab shells was purchased from COMBIO (Russia), and poly(vinyl
acetate) (PVAc), Mw¼ 350 kDa, was from PLASTPOLYMER (Russia).
Sodium hydroxide (98.5%, microprills with typical grain size
distribution of 0.5–1.2 mm> 93%) was from Merck (Germany). PVA
(Mowiol 66–100; Mw¼ 100 kDa; vinyl acetate units content 1 wt%) was
from Sigma–Aldrich (Germany).
. KGaA, Weinheim ADVANCED ENGINEERING MATERIALS 2011, 13, No. XX
RESEARCH
ARTIC
LE
D. Zaytseva-Zotova et al./Biocompatible Smart Microcapsules Based on Chitosan-Poly(vinyl alcohol) . . .
Cell Cultures
A number of mammalian cell lines were used in this study, namely
Siberian mountain goat kidney cell line (PSGK-60); baby hamster
kidney cells (BHK-21); rat-mouse hybridoma cells (1D2) producing
MAbs against IgG heavy chain; a mouse macrophage-like cell line
(P388D1); mouse melanoma cells (M3); human breast adenocarcinoma
cell line (MCF-7). We also used myeloma cells (Sp2/0), and two
human T-lymphoblastic leukemia cell lines (CCRF-CEM and
camptothecin resistant CEM/C1 subline).
PSGK-60 cells were cultured in MEM (Sigma–Aldrich, Germany)
while other cell lines were cultivated in DMEM (Sigma–Aldrich,
Germany) in CO2- incubator (HERAEUS B5060 EK/CO2) at 37 8C.
All culture media were supplemented with 1% gentamicin from
Akrihin (Russia) and 10% fetal bovine serum (FBS) from HyClone
(USA).
Synthesis and Characterization of Chitosan-g-PVA Copolymers
Two graft copolymers of chitosan and PVA, i.e., chitosan-g-PVA1
and chitosan-g-PVA20, having PVA/chitosan molar ratio 0.92 and
20.5, respectively, were obtained by solid-state synthesis as described
earlier [27]. Briefly, PVAc and chitin solid mixture (PVAc/chitin molar
ratio of 1.4 or 3) was processed with a semiindustrial corotating
twin-screw extruder (ZE 40A� 40D UTS, Berstorff, Germany) in the
presence of sodium hydroxide at 60 8C. The extruder has a variable set
of processing elements providing a high shear strain and a powerful
dispersive action. To remove low molecular weight compounds, the
prepared blends were exposed to a water/organic mixture (ethanol/
ethyl acetate/water) for extraction for 48 h followed by electrodialysis
in an aqueous solution for 1–2 d. After filtration, the sample solutions
were frozen and lyophilized at�10 toþ30 8C up to moisture content of
2–3%. Formation of chitosan-g-PVA copolymers was confirmed by
Fourier transform infrared spectroscopy (FTIR), gel penetration
chromatography (GPC), and elemental analysis.
To analyze the samples by FTIR, thin films (5–10 mm thickness)
were prepared by casting 2 wt% copolymer aqueous solutions onto
glass substrates. The cast solutions were dried at 50 8C for 2 h. To
prepare model blend films, PVA aqueous solution (10 wt%) and
previously obtained chitosan (Mw¼ 60 kDa; N-acetylated units
content 8 wt%) solution in 0.33 M acetic acid solution (10%) were
mixed. The formed films containing chitosan acetate were incubated
in a 1 M sodium hydroxide solution for 1 h, then carefully washed with
deionized water, and dried. To estimate the chitosan content in the
obtained products, a model blend film containing 20 wt% of chitosan
was used. Glucosamine content was calculated from an intensity ratio
of the bands assigned to chitosan �NH2 bending at 1 597 cm�1 and to
PVA�CH2� bending at 850 cm�1. The IR-spectra were recorded in an
absorbance mode at a resolution of 4 cm�1 and processed with Win-IR
software v. 4 (Bio-Rad Digilab Division). All the spectra were
normalized using the composite C�O band stretching vibrations of
the pyranose ring at 1 075 cm�1 as an internal standard.
The average Mw of the samples was determined by GPC on
Agilent 1200 (PLaquel – OH 40 column, pre-calibrated with
dextran standards, a flow rate of 1 mL �min�1, 25 8C). A solution
sample (0.2 wt%) in the eluent (H2Oþ 0.02% NaN3) was used. Relative
copolymer amounts were determined by means of an online refractive
index detector.
Glucosamine contents for chitosan and the both copolymers
were also calculated from the results of elemental analysis using C/N
ratio.
ADVANCED ENGINEERING MATERIALS 2011, 13, No. XX � 2011 WILEY-VCH Ve
Entrapment of Cells in Microcapsules and Cell Cultivation
Cell encapsulation was performed as described earlier [9], with a
minor modification. Cell precipitate (1–6� 106 cells) was mixed with a
sterilized NaAlg solution (2 wt%, 2 mL), and the mixture was added
through the needle (0.4 mm in diameter) into a CaCl2 solution
(0.5 wt%) using a special device with a coaxial air flow (2� 105 Pa) [28].
The obtained calcium alginate (CaAlg) hydrogel microbeads were
incubated with chitosan-g-PVA copolymer or oligochitosan solution
(25 mL, 0.1–1.2 wt%, 5–10 min), in order to form a polyelectrolyte
membrane on the microbead surface. Then the microbeads were
washed three times with a physiological solution (0.9 wt% NaCl).
To get hollow microcapsules, the microbeads were incubated in an
EDTA solution (50� 10�3M, 10 min), then washed again with the
physiological solution, and finally transferred to the culture medium.
The encapsulated cells were cultivated for 3–4 weeks to generate cell
aggregates (multicellular spheroids) within the microcapsules.
To measure the concentration of microencapsulated cells, micro-
capsule aliquots (0.1 mL slurry) were mechanically destroyed by
pipetting up and down rapidly. By using pipette it was possible to
destroy not only microcapsule membrane but also all cell aggregates
formed inside microcapsules and to get single cells. Then the released
single cells were stained with Trypan Blue and calculated in a
Fuchs–Rosenthal hemocytometer. All the experiments were repeated
three times, and the data were expressed as means� standard
deviations.
All the solutions for cell encapsulation were prepared in a
physiological solution.
Empty microcapsules (without cells) were prepared in the same
way as described above. The microcapsule size distribution and the
membrane thickness were calculated using optical microscopy
(Reichert Microstar 1820E, Germany).
Determination of Monoclonal Antibodies
Concentration of MAbs produced by encapsulated 1D2 hybridoma
cells in culture medium was examined by ELISA. The mouse IgG
antibody were added in 96-well plates (NUNC, Denmark) (2 mg in
100 mL �PBS �well�1) and incubated overnight at 4 8C. Then non-
specific binding sites were blocked with 200 mL of a buffer solution
(1 wt% BSA in 0.2 M PBS containing 0.05 wt% Tween-20), pH 7.2, at
37 8C for 1 h. Then the wells were washed with PBS four times. Then
aliquots (100 mL) of culture medium samples were added and
incubated at 37 8C for 1 h. After washing with PBS, aliquots
(100 mL) of a horseradish peroxidase-linked goat anti-rat IgG
conjugate (diluted to 1:10 in PBS containing 0.05 wt% Tween-20)
were added. Finally, the plates were incubated at 37 8C for 45 min.
Then 0.4 mg �mL�1 2,20-azino-bis(3-ethylbenzthiazoline-6-sulphonic
acid) was added to each well for detection. After 15 min the reaction
was stopped with 2 M H2SO4 solution, and the absorbance was
measured using microplate reader (Multiscan MCC/340) at 450 nm.
Evaluation of Methotrexate Cytotoxicity
After long-term cultivation (28 d) of MCF-7 cells in microcapsules
the obtained microcapsulated MTS were transferred into 96-well
plates (Nunc, Denmark) and incubated with a set of MTX solutions to
get final MTX concentrations of 1, 2, 10, 50, and 100� 10�9M. The
microcapsule aliquot (100 mL slurry) was mixed with the cultivation
medium (150 mL) supplemented with 10% FBS and MTX of
the appropriate concentration, and then incubated in a 5% CO2
atmosphere at 37 8C for 48 h. The monolayer cell culture
rlag GmbH & Co. KGaA, Weinheim http://www.aem-journal.com B7
RESEARCH
ARTIC
LE
D. Zaytseva-Zotova et al./Biocompatible Smart Microcapsules Based on Chitosan-Poly(vinyl alcohol) . . .
(5� 105 cells �mL�1) was used as control. The cell viability was
calculated after Trypan Blue dye staining using the Fuchs–Rosenthal
hemocytometer. The cytotoxicity was expressed as cell viability using
the following formula: Cell viability (%)¼ [viable cells concentration
in the experiment/viable cells concentration in the control)]� 100.
Received: March 1, 2011
Final Version: April 15, 2011
[1] A. Murua, A. Portero, G. Orive, R. M. Hernandez, M. de
Castro, J. L. Pedraz, J. Controlled Release 2008, 132, 76.
[2] F. Lim, A. M. Sun, Science 1980, 210, 908.
[3] a) B. Kulseng, B. Thu, T. Espevik, G. Skjak-Braek, Cell
Transplant. 1997, 6, 387; b) M. Brissova, I. Lacik,
A. C. Powers, A. V. Anilkumar, T. Wang, J. Biomed. Mater.
Res. 1998, 39, 61.
[4] M. Peirone, C. J. D. Ross, G. Hortelano, J. L. Brash,
P. L. Chang, J. Biomed. Mater. Res. 1998, 42, 587.
[5] a) Q. Wang, S. Li, Y. Xie, W. Yu, Y. Xiong, X. Ma,
Q. Yuan, Hepatol. Res. 2006, 35, 96; b) G. Mazzoleni,
D. Di Lorenzo, N. Steimberg, Genes Nutr. 2009, 4, 13.
[6] P. de Vos, M. Spasojevic, M. M. Faas, Adv. Exp. Med. Biol.
2010, 670, 38.
[7] O. Lindvall, L. U. Wahlberg, Exp. Neurol. 2008, 209, 82.
[8] G. D. Nicodemus, S. J. Bryant, Tissue Eng. Part B Rev.
2008, 14, 149.
[9] a) E. A. Markvicheva, L. Bezdetnaya, A. Bartkowiak,
A. Marc, J. L. Gorgen, F. Guillemin, D. Poncelet, Chem.
Ind. 2003, 12, 585; b) A. M. Tsoy, D. S. Zaytseva-Zotova,
E. F. Edelweiss, A. Bartkowiak, J.-L. Goergen, E. L.
Vodovozova, E. A. Markvicheva, Biochem. (Moscow),
Suppl. Ser. B: Biochem. Chem. 2010, 4, 243.
[10] S. Schneider, P. J. Feilen, V. Slotty, D. Kampfner,
S. Preuss, S. Berger, J. Beyer, R. Pommersheim, Bioma-
terials 2001, 22, 1961.
[11] L. Lin, Y. Song, C. Song, P. Xu, C. Song, Clin. Med. J. 2003,
116, 1161.
[12] a) Y. Gao, J. Xu, B. Sun, H. C. Jiang, World J. Gastroenterol.
2004, 10, 2067; b) T. M. Rahman, C. Selden, M. Khalil,
I. Diakonov, H. J. Hodgson, Artif. Organs 2004, 28, 476.
[13] A. Paul, Y. Ge, S. Prakash, D. Shum-Tim, Regen. Med.
2009, 4, 733.
[14] J. Dubrot, A. Portero, G. Orive, R. M. Hernandez,
A. Palazon, A. Rouzaut, J. L. Perez-Gracia, S. Hervas-
B8 http://www.aem-journal.com � 2011 WILEY-VCH Verlag GmbH & Co
Stubbs, J. L. Pedraz, I. Melero, Cancer Immunol. I.
Immunother. 2010, 59, 1621.
[15] a) P. de Vos, M. Bucko, P. Gemeiner, M. Navratil,
J. Svitel, M. Faas, B. L. Strand, G. Skjak-Braek,
Y. A. Morch, A. Vikartovska, I. Lacik, G. Kollarikova,
G. Orive, D. Poncelet, J.-L. Pedraz, M. B. Ansorge-
Schumacher, Biomaterials 2009, 30, 2559; b) G. Orive,
A. R. Gascon, R. M. Hernandez, M. Igartua,
J. L. Pedraz, Trends Pharmacol. Sci. 2003, 24, 207.
[16] a) B. Carreno-Gomez, R. Duncan, Int. J. Pharm. 1997, 148,
231; b) B. L. Strand, G. Skjak-Braek, O. Gaserod, in
Fundamentals of Cell Immobilization Biotechnology (Eds:
V. Nedovic, R. Willaert), Kluwer Academic Publishers,
The Netherlands 2004, p. 165.
[17] A. Bartkowiak, D. Hunkeler, Ann. N. Y. Acad. Sci. 1999,
875, 36.
[18] a) A. Nilasaroya, L. A. Poole-Warren, J. M. Whitelock,
P. Jo Martens, Biomaterials 2008, 35, 4658;
b) L. V. Thomas, U. Arun, S. Remya, P. D. Nair, J. Mater.
Sci. Mater. Med. 2009, 1, 59.
[19] K. Tanaka, F. Toda, Chem. Rev. 2000, 100, 1025.
[20] a) P. Yu. Butyagin, Russ. Chem. Rev. 1994, 63, 965;
b) A. A. Zharov, in High-Pressure Chemistry and Physics
of Polymers (Ed: A. L. Kovarskii), CRC Press Inc, London,
Tokyo 1994, p. 265.
[21] E. V. Prut, A. N. Zelenetskii, Russ. Chem. Rev. 2001,
70, 65.
[22] S. Z. Rogovina, T. A. Akopova, G. A. Vikhoreva, J. Appl.
Polym. Sci. 1998, 70, 927.
[23] R. M. Sutherland, Science 1988, 240, 177.
[24] W. R. Inch, J. A. McCredie, R. M. Sutherland, Growth
1970, 34, 271.
[25] a) M. T. Santini, G. Rainaldi, P. L. Indovina, Int. J.
Radiat. Biol. 1999, 75, 787; b) S. Marchal, A. Fadloun,
E. D. Maugain, M. A. Hallewin, F. Guillemin,
L. Bezdetnaya, Biochem. Pharmacol. 2005, 69, 1167.
[26] a) G. Hamilton, Cancer Lett. 1998, 131, 29;
b) F. Pampaloni, E. G. Reynaud, E. H. Stelzer, Nat.
Rev. Mol. Cell Biol. 2007, 8, 839; c) L. G. Griffith,
M. A. Swartz, Nat. Rev. Mol. Cell Biol. 2006, 7, 211.
[27] A. N. Ozerin, A. N. Zelenetskii, T. A. Akopova,
O. B. Pavlova-Verevkina, L. A. Ozerina, N. M. Surin,
A. S. Kechek’yan, Polym. Sci. Ser. A 2006, 48, 638.
[28] O. E. Selina, A. A. Chinarev, P. S. Obukhova,
A. Bartkowiak, N. V. Bovin, E. A. Markvicheva, Russ.
J. Bioorg. Chem. 2008, 34, 468.
. KGaA, Weinheim ADVANCED ENGINEERING MATERIALS 2011, 13, No. XX