We’re sorry, something doesn't seem to be working properly.
Please try refreshing the page. If that doesn't work, please contact us so we can address the problem.
Comparison of a xeno-free and serum-free culture system for human embryonic stem cells with conventional culture systems
- Dan Zhang†1,
- Qingyun Mai†1,
- Tao Li1,
- Jia Huang1,
- Chenhui Ding1,
- Mengxi Jia1,
- Canquan Zhou1Email author and
- Yanwen Xu1Email author
© The Author(s). 2016
- Received: 21 February 2016
- Accepted: 10 June 2016
- Published: 30 July 2016
Elimination of all animal components during derivation and long-term culture of human embryonic stem cells (hESCs) is necessary for future applications of hESCs in clinical cell therapy.
In this study, we established the culture system of xeno-free human foreskin fibroblast feeders (XF-HFF) in combination with chemically defined medium (CDM). XF-HFF/CDM was compared with several conventional culture systems. The hESCs cultured in different media were further characterized through karyotype analysis, pluripotency gene expression, and cell differentiation ability.
The hESCs in the XF-HFF/CDM maintained their characteristics including typical morphology and stable karyotype. In addition, hESCs were characterized by fluorescent immunostaining of pluripotent markers and teratoma formation in vivo. RT-PCR analysis shown that the stem cell markers OCT3/4, hTERT, SOX2, and Nanog were present in the cell line hESC-1 grown on XF-HFF/CDM. Furthermore, the results of cell growth and expression of bFGF, Oct-4, and hTERT indicated that XF-HFF/CDM had better performance than human serum-matrix/CDM and XF-HFF/human serum.
The comparison of different xeno-free culture conditions will facilitate clarifying the key features of self-renewal, pluripotency, and derivation and will shed light on clinic applications of hESCs.
- Human embryonic stem cell
- Xeno-free and serum-free culture system
- Chemically defined medium
- Human foreskin fibroblast cells
Human embryonic stem cells (hESCs) can differentiate into various cell types and possess great potential for cell-replacement therapy including treatment for diabetes, cardiac infarction, and neurodegenerative diseases [1, 2]. The major challenge for the clinical application of hESCs are animal-derived products and undefined factors during in-vitro establishment and expansion of the cells. Nevertheless, hESCs are conventionally cultured on feeder cell layers, of which mouse embryonic fibroblasts (MEFs) are the most common and present several unknown animal-derived products . The risk of graft rejection and immunoreactions will be increased greatly, demonstrating that a xeno-support system sets a limitation for the therapeutic potential of hESCs to a great extent [4–6]. Optimization and standardization of a fully defined xeno-free culture for hESCs is therefore urgent.
Xeno-free culture conditions continue to evolve to avoid exposure to animal-derived materials [7–9]. However, some issues including chromosomal abnormalities in hESCs arise due to more demanding growth conditions . On the contrary, feeder-free cultures generally present a higher degree of spontaneous differentiation in comparison with conventional cultures, signifying that higher concentration of exogenous basic fibroblast growth factor (bFGF) is required and feeder-free derivation is not optimal for developing transplantable hESC derivatives .
Considerable progress has been made towards maintaining hESC cultures since human feeder cells were proposed . Several researchers have proved the ability to culture hESCs on human feeder cells which were isolated from human tissues, including adult marrow tissues , fetal muscle, fetal skin, human placental fibroblasts , and human endometrial cells . Some contributions have been made to derive and culture new human foreskin feeders (hFFs) [16–18].
Other groups have attempted to culture hESCs in chemically defined as well as xeno-free conditions. Some studies have claimed the defined media can retain hESCs successfully in their pluripotent state [19, 20], while other studies have contradicted this . Chin et al.  described the defined StemPro and mTeSR1 media without feeder and the xeno-free HEScGRO medium with hFFs for hESC growth. Further efforts should be made to culture hESCs in anticipation of future applications.
In this study, we evaluated whether xeno-free human foreskin fibroblast feeders (XF-HFF) combined with chemically defined medium (CDM) could be successfully used in long-term maintenance of undifferentiated hESCs. At the same time, the characteristics of hESCs grown under these conditions were assessed after prolonged culture, including their unlimited and undifferentiated proliferative ability, maintenance of normal karyotype in long-term culture, and their developmental potential to differentiate into representative tissues of all three embryonic germ layers. In addition, the efficacy of this culture system was compared with other culture conditions with respect to cell growth and undifferentiated states.
Human material and ethics statement
The design and performance of this study conformed to the ethical standards of the Helsinki Declaration and our national legislation. This study was approved by the Medical Ethical Committee of The First Affiliated Hospital, Sun Yat-sen University. An informed consent form was signed by the participant or the legal guardian for children after receiving a written description of the study.
Human blood was obtained from healthy donors, infant foreskin from circumcised infants, and discarded human embryos from donors undergoing clinical in-vitro fertilization treatment. Patients who donated blood and foreskins were negative for HIV, hepatitis B and C, and syphilis.
Preparation of xeno-free human foreskin fibroblast cells (XF-HFF)
Human serum (HS) and XF-HFF were prepared as described previously . XF-HFF were cultured in 90 % Dulbecco’s modified Eagle’s medium (DMEM; Invitrogen, Carlsbad, CA, USA) supplied with 10 % HS, 1 % penicillin–streptomycin (PS; HyClone Laboratories, Inc., Logan, UT, USA). The medium was changed daily. XF-HFF were normally passaged by TrypLE Select (Invitrogen) at a 1:8–1:10 split ratio every 3–5 days.
For preparation of feeder layers, XF-HFF were treated with mitomycin C (Sigma, St. Louis, MO, USA) for 2.5 h, and the treated cells were reseeded at 75,000 cells/cm2.
Four culture systems were described in this study as follows: XF-HFF combined with CDM (HEScGRO; Chemicon, Billerica, MA, USA) (XF-HFF/CDM group), XF-HFF combined with 20 % HS medium (XF-HFF/HS group), HS-matrix coated on plates without feeder layers combined with CDM (HS-matrix/CDM group), and xeno-contained human foreskin fibroblast feeders (XC-HFF) combined with 20 % KnockOut Serum Replacement (KSR medium) (XC-HFF/KSR group). Two hESC lines (hESC-1, hESC-2) derived in our laboratory were propagated for 25 passages in the XC-HFF/KSR group, and were then transferred to the other three hESC culture systems.
Total RNA was extracted using the RNeasy kit (Qiagen, Valencia, CA, USA). Approximately 500 ng of RNA template was reverse-transcribed into cDNA using the SuperScript III First-Strand Synthesis System for RT-PCR (Invitrogen). The cDNA was amplified by PCR using the Accuprime Taq DNA polymerase system (Invitrogen). The housekeeping gene glyceraldehyde-3-phosphate dehydrogenase (GAPDH) was used as an internal positive control. PCR products were run on a 2 % agarose gel, stained with ethidium bromide and visualized by UV illumination.
The primers sequences were: octamer-binding transcription factor Oct-4, 5′-GAAGGTATTCAGCCAAAC-3′ and 5′-CTTAATCCAAAAACCCTGG-3′; Nanog, 5′-GATCGGGCCCGCCACCATGAGTGTGGATCCAGCTTG-3′ and 5′-GATCGAGCTCCATCTTCACACGTCTTCAGGTTG-3′; human telomerase reverse transcriptase (hTERT), 5′-CGGAAGAGTGTCTGGAGCAAGT-3′ and 5′-GAACAGTGCCTTCACCCTCGA-3′; SOX2, 5′-CGGAAAACCAAGACGCTCA-3′ and 5′-GCCGTTCATGTAGGTCTGCG-3′; GAPDH, 5′-GTCAGTGGTG GACCTGACCT-3′ and 5′-CACCACCCTGTTGCTGTAGC-3′.
Karyotype analysis of hESCs
The genetic stability of hESCs grown in the xeno-free culture system was determined by examining the karyotype using a standard G-banding procedure. Briefly, cells were incubated with colcemid, trypsinized, and then resuspended. The samples were then fixed onto the prepared slides to make the chromosome spreads. The dried slides were baked for 90 min at 80 °C, treated with 0.05 % trypsin for 30 sec to 2 min, and then stained with Giemsa and Leishman’s solution.
Teratomas were generated by intramuscular injection of undifferentiated hESCs (6 × 106 cells) into the hind limb of severe combined immunodeficient (SCID) mice. The injected mice were sacrificed at 8 weeks post injection, and the resulting teratomas were fixed with 4 % paraformaldehyde and embedded with paraffin. The samples were then stained with hematoxylin and eosin, and observed under a light microscope.
Growth curve analysis
hESCs were plated at a density of 40,000 cells per well and cultured in different medium. The number of cells was counted using a hemacytometer at days 3, 5, and 7 to obtain a growth curve.
hESC cultures were rinsed with PBS and then incubated with 0.5 mM EDTA (Sigma) at 37 °C for 5–8 min. The dissociated cells were rinsed twice in PBS for further analysis. Single cells were then blocked with 10 % goat serum (HyClone) for 15 min. All staining procedures were performed using buffer containing 2 % goat serum, 0.1 % sodium azide (Sigma), and 2 mM EDTA in PBS. The blocked cells were incubated with primary antibodies (stage-specific embryonic antigen SSEA-4 or tumor rejection antigen TRA-1-60, 1:20; Chemicon, Temecula, CA) for 30 min at 4 °C followed by three washes in PBS. The cells were then probed with a 1:100 dilution of Alexa-488-conjugated goat F(ab′)2 anti-mouse immunoglobulin (Ig)G3 or phycoerythrin-conjugated goat F(ab′)2 anti-mouse IgM (both from Invitrogen) for 30 min in the dark at 4 °C. The cells were washed once and resuspended for analysis in staining buffer containing 1 μg/ml of propidium iodide (Sigma) to identify nonviable cells. Flow cytometry analysis was performed using a FACS Calibur flow cytometer (BD Bioscience, San Jose, CA, USA).
Quantification of Oct-4 and hTERT mRNA
RNA was isolated from hESC populations using an RNeasy kit (Qiagen), according to the manufacturer’s protocol. Extracted RNA was subsequently treated with DNA-free DNase I (Ambion, Austin, TX, USA). Real-time PCR amplification was performed on an Applied Biosystems International 7500 Sequence Detection System (Applied Biosystems, Foster City, CA, USA). The TaqMan one-step RT-PCR master mix (Applied Biosystems) was applied with the following reaction conditions: RT at 48 °C for 30 min; denaturation and AmpliTaq gold activation at 95 °C for 10 min; and amplification for 40 cycles at 95 °C for 15 sec and at 60 °C for 1 min. All reactions were performed in triplicate. The Oct-4 sequences were designed by Applied Biosystems Primer Express software: forward primer, 5′-GCA ACC TGG AGA ATT TGT TCC T-3′; reverse primer, 5′-CCA CAC TCG GAC CAC ATC CT-3′; and probe, FAM-5′-CAG TGC CCG AAA CCC ACA CTG C-3′-TAMRA. The 18 s and hTERT probe and primers were purchased from Applied Biosystems. Relative quantification of gene expression between multiple samples was achieved by normalization against endogenous18S ribosomal RNA using the △△CT method of quantification (Applied Biosystems). Relative fold difference in gene expression was calculated as 2–(ΔΔCT).
The characterization of hESCs grown in animal-free conditions was carried out by measuring the expression of specific pluripotency markers including: SSEA-3, SSEA-4, SSEA-1, TRA-1-60, and TRA-1-81. hESCs were washed once in PBS and fixed in 4 % paraformaldehyde (DGCS biotech) at room temperature for 15 min. The cells were then blocked in PBST (PBS containing 0.1 % Triton 100 (DGCS) and 0.25 % normal donkey serum (Jackson Immuno Research Laboratories, West Baltimore, USA)) at room temperature for 1 h. Primary and secondary antibodies were diluted in PBST. Cells were incubated with primary antibodies at 4 °C for 2 h, followed by three rinses and then incubation with secondary antibodies at room temperature for 1 h. Cells were then washed three times in PBS prior to imaging. Stained preparations were examined under a Nikon Eclipse TE-2000 U fluorescence microscope (Nikon, Tokyo, Japan).
All data were obtained from three replicate experiments. Values from all experiments were expressed as the mean ± standard deviation (SD). Student’s t test and a chi-square test were employed to analyze the statistical differences between culture groups. The analyses were performed using SPSS software version 10 (SPSS Inc., Chicago, IL, USA). p < 0.05 was considered statistically significant.
Characterizations of hESCs in the XF-HFF/CDM culture system
hESCs cultured in XF-HFF/CDM exhibit normal cell morphologies
hESCs cultured in XF-HFF/CDM express stem cell markers
Karyotype of hESCs cultured in XF-HFF/CDM
hESCs cultured in XF-HFF/CDM are pluripotent
Comparison of different hESC culture systems
Culture efficacy of XF-HFF/CDM conditions and other culture conditions on the survival and differentiation rates of hESCs after transferring four passages
Colony formation rate (%)a
Differentiation rate (%)b
91.25 ± 2.22
6.00 ± 1.83
26.5 ± 2.08*
85.00 ± 3.60*
77.75 ± 2.21*
86.00 ± 3.37*
93.75 ± 2.22
5.50 ± 2.02
Morphology of hESCs cultured with the other three culture media
Based on morphology, the colonies in XF-HFF/HS and HS-matrix/CDM became thinner and some lost their regular shapes and defined borders compared with that seen in XC-HFF/KSR by bright-field microscopy (Fig. 1c–e). In the XF-HFF/HS group and the HS-matrix/CDM group, hESCs lost their undifferentiated morphology and showed a high rate of differentiation and a low rate of colony formation (Fig. 1c,d). In addition, they were unable to maintain their undifferentiated states over six passages. The results indicated that XF-HFF/CDM had an advantage over XF-HFF/HS and HS-matrix/CDM in maintaining the pluripotency of hESCs.
Growth of hESCs cultured with the other three culture media
Undifferentiated states of hESC clones under different culture systems
The undifferentiated states of hESC clones under different culture systems were compared by analyzing the expression levels of SSEA-4 and TRA-1-60 by flow cytometry (Fig. 5b). Consistent with the morphologic observations, both CDM-cultured and KSR medium-cultured hESC clones on hFFs expressed high levels of undifferentiated surface marker expression. hESCs cultured in HS-matrix with CDM or HS medium on hFFs, however, downregulated these markers.
We performed quantitative RT (qRT)-PCR to confirm the expression levels of hESC markers. OCT-4 and hTERT were expressed in undifferentiated hESCs and downregulated upon differentiation. Figure 6b shows that hESCs in HS-matrix conditions or HS medium conditions expressed low levels of OCT-4 and hTERT. The expression level of the pluripotency marker OCT-4 under XF-HFF/CDM was twofold higher than that under HS-matrix conditions or HS medium conditions. Measurement of hTERT expression by RT-PCR in four culture systems showed that the changing trend was almost the same as that of OCT-4 (Fig. 6b). The hESCs maintained in the XF-HFF/CDM system therefore had relatively high levels of OCT-4 and hTERT, resembling undifferentiated hESCs maintained on XC-HFF/KSR.
As a renewable cell source for future regenerative medicine applications, the derivation, passaging, and culture of hESCs have attracted widespread attention . To generate therapeutically safe and usable hESC derivatives for clinical cell treatment, all animal-derived materials which are a potential risk for infection transmitted by animal pathogens must be eliminated during the process .
The major sources of xeno-contamination are the presence of animal feeders and the use of either FBS or serum replacement (SR) in the culture medium . Many groups have previously claimed successful culture of hESCs on hFFs and other feeders [7, 12, 14, 25–28]. Hovatta et al.  used commercially available human foreskin fibroblasts for hESC propagation. Crook et al.  proposed the proof of concept for the generation of six clinical-grade hESC lines using hFFs as feeder cells. hFFs isolated from infant foreskin have a distinct advantage over MEFs. In addition to the xenobiotic issue, hFFs can be cultured for up to 62 passages before senescence, while MFFs can only be propagated for five passages [7, 30]. Moreover, little ethical concern is considered over the acquirement of foreskin tissue for the generation of feeder cells.
Another obstacle to overcome was the presence of FBS or SR in the culture medium. Several studies described the use of HS as serum supplement to culture hESCs. However, it has been proved previously that commercial xeno-free SRs and human sera are inappropriate for long-term culture of hESCs . Some attempts to use HS as a medium supplement failed due to spontaneous differentiation [12, 26, 31]. It is important to point out that HS may be involved in the interactions between secreted factors from the feeder cells. Therefore, it is highly desirable to employ defined components rather than complex mixtures [32–35]. The establishment of a chemically defined xeno-free and feeder-free culture system is advantageous for exact identification of factors secreted by feeder layers or signal pathways existing in them. Thus, xeno-free commercially available CDM was employed in the culture system.
Our data demonstrate that hESCs can be successfully derived and cultured long term in the XF-HFF/CDM system while maintaining their undifferentiated state. Furthermore, teratoma analysis demonstrated that hESCs maintain their pluripotency and differentiation potential, which were comparable with hESCs cultured in the conventional hESC culture medium. The use of CDM with hFF cells has been described previously . On the basis of that work, we further presented the differences of culture systems for hESCs. We tested four culture systems and two hESC lines, and little variation was observed between hESCs cultured in CDM and KSR medium in maintaining undifferentiated states of hESCs. On the other hand, data obtained by flow cytometry and qRT-PCR demonstrated that feeder cells supported the growth of undifferentiated hESCs more efficiently than HS-matrix when cells were presented in CDM. The HS-matrix, which contains hyaluronic acid, fibronectin, and vitronectin, as well as other unknown human factors, supports the attachment and growth of undifferentiated cells . Stojkovic et al.  suggested that HS used as a matrix maintained pluripotency and genomic stability of hESCs. Meng et al.  pointed that extracellular matrix isolated from foreskin fibroblasts has an advantage in the process of long-term xeno-free hESC culture. However, feeder-free cultures usually presented a higher degree of spontaneous differentiation than conventional culture along with a higher concentration of exogenous bFGF, which indicated that feeder-free derivation and culture were not suitable for developing transplantable hESC derivatives . The results in this manuscript also proved that the HS-matrix/CDM system could not maintain the undifferentiated state and differentiated potential of hESCs. Although the molecular and developmental mechanisms controlling the pluripotency and differentiation of hESCs are largely unknown, feeder cells may provide a better, more stable environment, and thus they can secrete the unique proteins that participate in cell growth, extracellular matrix formation, and remodeling [1, 39].
The results demonstrated that CDM provided an effective replacement for HS medium, comparable with KSR medium, to support hESC self-renewal and pluripotency. This observation suggests that CDM and KSR medium culture conditions supply similar growth factors or signal pathways for hESC growth. CDM is more suitable than serum-containing medium for studies that aimed at identifying the exogenous signals required for undifferentiated hESC growth. XF-HFF/HS were unable to maintain undifferentiated of hESCs in long-term growth.
Exogenous bFGF has been identified as a key factor involved in self-renewal of hESCs [40–43], and some studies have indicated that FGF proteins are sensitive to thermal denaturation, while fibroblasts likely secrete either protease inhibitors or binding proteins that modulate bFGF stability [42, 44]. In our work, we found that bFGF was unstable in 37 °C culture conditions. Although the concentrations of bFGF declined in all culture conditions, they were higher in cofeeder conditions than in feeder-free conditions. The data indicated that fibroblast is likely to secrete some proteins which modulate the stability of bFGF , and also indicated that the stability of bFGF was not the only factor responsible for the successful culture of hESCs.
Lysophosphatidic acid (LPA) as the key lipid is a simple phospholipid mediator which plays an important role in the regulation of cell proliferation, migration, and survival of multiple cell types [45, 46]. Todorova et al.  proposed that LPA was involved in the expression of the Ca2+-dependent early response gene c-myc, which was a key gene implicated in ESC self-renewal and pluripotency. Therefore, LPA increased the proliferation rate of mESCs. Liu et al. demonstrated that LPA induced the expression of the erythroid biomarkers in cultured human hematopoietic stem cells (hHSCs) under plasma-free conditions. In addition, LPA was also reported to enhance osteogenic differentiation of human mesenchymal stem cells . These results suggested that LPA may play a critical role in cell fate determination. Hence, we suspected that HFF-1 cells could secrete LPA to support the long-term culture.
We have reported the development of a xeno-free and serum-free method for culturing hESCs. The hESCs in the established XF-HFF/CDM culture system maintained their properties, such as typical morphology, pluripotency, capacity to form three germ layers in vivo, and stable karyotype. The results show that the XF-HFF/CDM culture medium is applicable for further optimization of xeno-free establishment, culture, and differentiation of stem cells. Future studies should focus on the comparison of different xeno-free culture conditions and on validation of these conditions to demonstrate the key features of self-renewal, pluripotency, and derivation.
bFGF, basic fibroblast growth factor; CDM, chemically defined medium; DMEM, Dulbecco’s modified Eagle’s medium; ELISA, enzyme-linked immunosorbent-based assay; GAPDH, glyceraldehyde-3-phosphate dehydrogenase; hESC, human embryonic stem cell; hFF, human foreskin feeder; HS, human serum; hTERT, human telomerase reverse transcriptase; KSR, KnockOut Serum Replacement; LPA, lysophosphatidic acid; MEF, mouse embryonic fibroblast; OCT, octamer-binding transcription factor; qRT-PCR, quantitative RT-PCR; SCID, severe combined immunodeficient; SR, serum replacement; SSEA, stage-specific embryonic antigen; Tra, tumor rejection antigen; XC-HFF, xeno-contained human foreskin fibroblast feeders; XF-HFF, xeno-free human foreskin fibroblast feeders
This work was supported by Guangdong Provincial Key Laboratory of Reproductive (2012A061400003) and National Natural Science Foundation of China (NO:81270750 and NO:81300481). The authors thank Prof. Chen for his help with the karyotype analysis in the Department of Medical Genetics of Basic Medical College, and Caixia Liu and Pingping Hong for the hESC-passaging method.
DZ carried out the teratoma formation studies, participated in the quantification of Oct-4 and hTERT mRNA assays, and drafted the manuscript. QM carried out the immunofluorescence assays and revised the manuscript. TL participated in the quantification of Oct-4 and hTERT mRNA assays and drafted the manuscript. JH carried out the karyotype of hESC studies and drafted the manuscript. DH participated in growth curve analysis and revised the manuscript. BC and participated in the design of the study, performed the statistical analysis, and helped to revise the manuscript. CZ and YX conceived of the study, participated in its design and coordination, and helped to draft the manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- Ellerström C, Strehl R, Moya K, Andersson K, Bergh C, Lundin K, et al. Derivation of a xeno‐free human embryonic stem cell line. Stem Cells. 2006;24:2170–6.View ArticlePubMedGoogle Scholar
- Yao S, Chen S, Clark J, Hao E, Beattie GM, Hayek A, et al. Long-term self-renewal and directed differentiation of human embryonic stem cells in chemically defined conditions. Proc Natl Acad Sci U S A. 2006;103:6907–12.View ArticlePubMedPubMed CentralGoogle Scholar
- Choo AB, Padmanabhan J, Chin AC, Oh SK. Expansion of pluripotent human embryonic stem cells on human feeders. Biotechnol Bioeng. 2004;88:321–31.View ArticlePubMedGoogle Scholar
- Martin M, Muotri A, Gage F, Varki A. Human embryonic stem cells express an immunogenic nonhuman sialic acid. Nat Med. 2005;11:228–32.View ArticlePubMedGoogle Scholar
- Lu J, Hou R, Booth CJ, Yang SH, Snyder M. Defined culture conditions of human embryonic stem cells. Proc Natl Acad Sci U S A. 2006;103:5688–93.View ArticlePubMedPubMed CentralGoogle Scholar
- Skottman H, Hovatta O. Culture conditions for human embryonic stem cells. Reproduction. 2006;132:691–8.View ArticlePubMedGoogle Scholar
- Amit M, Shariki C, Margulets V, Itskovitz-Eldor J. Feeder layer- and serum-free culture of human embryonic stem cells. Biol Reprod. 2004;70:837–45.View ArticlePubMedGoogle Scholar
- Meng G, Liu S, Rancourt DE. Synergistic effect of medium, matrix, and exogenous factors on the adhesion and growth of human pluripotent stem cells under defined, xeno-free conditions. Stem Cells Dev. 2011;21:2036–48.View ArticleGoogle Scholar
- Miwa H, Hashimoto Y, Tensho K, Wakitani S, Takagi M. Xeno-free proliferation of human bone marrow mesenchymal stem cells. Cytotechnology. 2012;64:301–8.View ArticlePubMedGoogle Scholar
- Draper JS, Smith K, Gokhale P, Moore HD, Maltby E, Johnson J, et al. Recurrent gain of chromosomes 17q and 12 in cultured human embryonic stem cells. Nat Biotechnol. 2004;22:53–4.View ArticlePubMedGoogle Scholar
- Kim SJ, Cheon SH, Yoo SJ, Kwon J, Park JH, Kim CG, et al. Contribution of the PI3K/Akt/PKB signal pathway to maintenance of self-renewal in human embryonic stem cells. FEBS Lett. 2005;579:534–40.View ArticlePubMedGoogle Scholar
- Richards M, Fong CY, Chan WK, Wong PC, Bongso A. Human feeders support prolonged undifferentiated growth of human inner cell masses and embryonic stem cells. Nat Biotechnol. 2002;20:933–6.View ArticlePubMedGoogle Scholar
- Cheng L, Hammond H, Ye Z, Zhan X, Dravid G. Human adult marrow cells support prolonged expansion of human embryonic stem cells in culture. Stem Cells. 2003;21:131–42.View ArticlePubMedGoogle Scholar
- Genbacev O, Krtolica A, Zdravkovic T, Brunette E, Powell S, Nath A, et al. Serum-free derivation of human embryonic stem cell lines on human placental fibroblast feeders. Fertil Steril. 2005;83:1517–29.View ArticlePubMedGoogle Scholar
- Lee JB, Lee JE, Park JH, Kim SJ, Kim MK, Roh SI, et al. Establishment and maintenance of human embryonic stem cell lines on human feeder cells derived from uterine endometrium under serum-free condition. Biol Reprod. 2005;72:42–9.View ArticlePubMedGoogle Scholar
- Fletcher JM, Ferrier PM, Gardner JO, Harkness L, Dhanjal S, Serhal P, et al. Variations in humanized and defined culture conditions supporting derivation of new human embryonic stem cell lines. Cloning Stem Cells. 2006;8:319–34.View ArticlePubMedGoogle Scholar
- Meng G, Liu S, Krawetz R, Chan M, Chernos J, Rancourt DE. A novel method for generating xeno-free human feeder cells for human embryonic stem cell culture. Stem Cells Dev. 2008;17:413–22.View ArticlePubMedGoogle Scholar
- Stacey GN, Cobo F, Nieto A, Talavera P, Healy L, Concha A. The development of “feeder” cells for the preparation of clinical grade hES cell lines: challenges and solutions. J Biotechnol. 2006;125:583–8.View ArticlePubMedGoogle Scholar
- Liu Y, Song Z, Zhao Y, Qin H, Cai J, Zhang H, et al. A novel chemical-defined medium with bFGF and N2B27 supplements supports undifferentiated growth in human embryonic stem cells. Biochem Biophys Res Commun. 2006;346:131–9.View ArticlePubMedGoogle Scholar
- Li Y, Powell S, Brunette E, Lebkowski J, Mandalam R. Expansion of human embryonic stem cells in defined serumfree medium devoid of animal-derived products. Biotechnol Bioeng. 2005;91:688–98.View ArticlePubMedGoogle Scholar
- Rajala K, Hakala H, Panula S, Aivio S, Pihlajamaki H, Suuronen R, et al. Testing of nine different xeno-free culture media for human embryonic stem cell cultures. Hum Reprod. 2007;22:1231–8.View ArticlePubMedGoogle Scholar
- Chin ACP, Padmanabhan J, Oh SKW, Choo ABH. Defined and serum-free media support undifferentiated human embryonic stem cell growth. Stem Cells Dev. 2009;19:753–61.View ArticleGoogle Scholar
- Hoffman LM, Carpenter MK. Characterization and culture of human embryonic stem cells. Nature Biotechnol. 2005;23:699–708.View ArticleGoogle Scholar
- Mallon BS, Park KY, Chen KG, Hamilton RS, McKay RD. Toward xeno-free culture of human embryonic stem cells. Int J Biochem Cell Biol. 2006;38:1063–75.View ArticlePubMedPubMed CentralGoogle Scholar
- Inzunza J, Gertow K, Strömberg MA, Matilainen E, Blennow E, Skottman H, et al. Derivation of human embryonic stem cell lines in serum replacement medium using postnatal human fibroblasts as feeder cells. Stem Cells. 2005;23:544–9.View ArticlePubMedGoogle Scholar
- Richards M, Tan S, Fong CY, Biswas A, Chan WK, Bongso A. Comparative evaluation of various human feeders for prolonged undifferentiated growth of human embryonic stem cells. Stem Cells. 2003;21:546–56.View ArticlePubMedGoogle Scholar
- Hovatta O, Mikkola M, Gertow K, Strömberg AM, Inzunza J, Hreinsson J, et al. A culture system using human foreskin fibroblasts as feeder cells allows production of human embryonic stem cells. Hum Reprod. 2003;18:1404–9.View ArticlePubMedGoogle Scholar
- Stojkovic P, Lako M, Stewart R, Przyborski S, Armstrong L, Evans J, et al. An autogeneic feeder cell system that efficiently supports growth of undifferentiated human embryonic stem cells. Stem Cells. 2005;23:306–14.View ArticlePubMedGoogle Scholar
- Crook JM, Peura TT, Kravets L, Boesman AG, Buzzard JJ, Horne R, et al. The generation of six clinical-grade human embryonic stem cell lines. Cell Stem Cell. 2007;1:490–4.View ArticlePubMedGoogle Scholar
- Meng GL, Zur Nieden NI, Liu SY, Cormier JT, Kallos MS, Rancourt DE. Properties of murine embryonic stem cells maintained on human foreskin fibroblasts without LIF. Mol Reprod Dev. 2008;75:614–22.View ArticlePubMedGoogle Scholar
- Koivisto H, Hyvärinen M, Strömberg AM, Inzunza J, Matilainen E, Mikkola M, et al. Cultures of human embryonic stem cells: serum replacement medium or serum-containing media and the effect of basic fibroblast growth factor. Reprod BioMed Online. 2004;9:330–7.View ArticlePubMedGoogle Scholar
- Nakagawa M, Taniguchi Y, Senda S, Takizawa N, Ichisaka T, Asano K, et al. A novel efficient feeder-free culture system for the derivation of human induced pluripotent stem cells. Sci Rep-UK. 2014;4:3594.Google Scholar
- Wang Q, Mou X, Cao H, Meng Q, Ma Y, Han P, et al. A novel xeno-free and feeder-cell-free system for human pluripotent stem cell culture. Protein Cell. 2012;3:51–9.View ArticlePubMedPubMed CentralGoogle Scholar
- Totonchi M, Taei A, Seifinejad A, Tabebordbar M, Rassouli H, Farrokhi A, et al. Feeder-and serum-free establishment and expansion of human induced pluripotent stem cells. Int J Dev Biol. 2010;54:877.View ArticlePubMedGoogle Scholar
- Rajala K, Lindroos B, Hussein SM, Lappalainen RS, Mattila M, Inzunza J, et al. A defined and xeno-free culture method enabling the establishment of clinical-grade human embryonic, induced pluripotent and adipose stem cells. PloS ONE. 2010;5:10246.View ArticleGoogle Scholar
- Uhm JH, Dooley NP, Kyritsis AP, Rao JS, Gladson CL. Vitronectin, a glioma-derived extracellular matrix protein, protects tumor cells from apoptotic death. Clin Cancer Res. 1999;5:1587–94.PubMedGoogle Scholar
- Stojkovic P, Lako M, Przyborski S, Stewart R, Armstrong L, Evans J, et al. Human-serum matrix supports undifferentiated growth of human embryonic stem cells. Stem Cells. 2005;23:895–902.View ArticlePubMedGoogle Scholar
- Meng G, Liu S, Li X, Krawetz R, Rancourt DE. Extracellular matrix isolated from foreskin fibroblasts supports long-term xeno-free human embryonic stem cell culture. Stem Cells Dev. 2010;19:547–56.View ArticlePubMedGoogle Scholar
- Prowse AB, McQuade LR, Bryant KJ, Van Dyk DD, Tuch BE, Gray PP. A proteome analysis of conditioned media from human neonatal fibroblasts used in the maintenance of human embryonic stem cells. Proteomics. 2005;5:978–89.View ArticlePubMedGoogle Scholar
- Vallier L, Alexander M, Pedersen RA. Activin/Nodal and FGF pathways cooperate to maintain pluripotency of human embryonic stem cells. J Cell Sci. 2005;118:4495–509.View ArticlePubMedGoogle Scholar
- Xu RH, Peck RM, Li DS, Feng X, Ludwig T, Thomson JA. Basic FGF and suppression of BMP signaling sustain undifferentiated proliferation of human ES cells. Nat Methods. 2005;2:185–90.View ArticlePubMedGoogle Scholar
- Levenstein ME, Ludwig TE, Xu RH, Llanas RA, Van Den Heuvel‐Kramer K, Manning D, et al. Basic fibroblast growth factor support of human embryonic stem cell self-renewal. Stem Cells. 2006;24:568–74.View ArticlePubMedGoogle Scholar
- Xu C, Rosler E, Jiang J, Lebkowski JS, Gold JD, O'Sullivan C, et al. Basic fibroblast growth factor supports undifferentiated human embryonic stem cell growth without conditioned medium. Stem Cells. 2005;23:315–23.View ArticlePubMedGoogle Scholar
- Eiselleova L, Peterkova I, Neradil J, Slaninova I, Hampl A, Dvorak P. Comparative study of mouse and human feeder cells for human embryonic stem cells. Int J Dev Biol. 2008;52:353–63.View ArticlePubMedGoogle Scholar
- Chiang CL, Chen SSA, Lee SJ, Tsao KC, Chu PL, et al. Lysophosphatidic acid induces erythropoiesis through activating lysophosphatidic acid receptor 3. Stem Cells. 2011;29:1763–73.View ArticlePubMedGoogle Scholar
- Costa M, Sourris K, Lim SM, Qing CY, Hirst CE, et al. Derivation of endothelial cells from human embryonic stem cells in fully defined medium enables identification of lysophosphatidic acid and platelet activating factor as regulators of eNOS localization. Stem Cell Res. 2013;10:103–17.View ArticlePubMedGoogle Scholar
- Todorova MG, FuentesE SB, Nadal A, Quesada I, et al. Lysophosphatidic acid induces Ca2+ mobilization and c-Myc expression in mouse embryonic stem cells via the phospholipase C pathway. Cell Signal. 2009;21:523–8.View ArticlePubMedGoogle Scholar
- Liu YB, Kharode Y, Bodine PVN, Yaworsky PJ, Robinson JA, et al. LPA induces osteoblast differentiation through interplay of two receptors: LPA1 and LPA4. J Cell Biochem. 2010;109:794–800.PubMedGoogle Scholar