Open Access

Biological impact of xeno-free chemically defined cryopreservation medium on amniotic epithelial cells

  • Toshio Miki1, 3Email author,
  • Wisia Wong3,
  • Elton Zhou3,
  • Anthony Gonzalez3,
  • Irving Garcia3 and
  • Brendan H. Grubbs2
Stem Cell Research & Therapy20167:8

DOI: 10.1186/s13287-015-0258-z

Received: 12 March 2015

Accepted: 4 December 2015

Published: 12 January 2016

Abstract

Background

Amnion-derived stem cells have been proposed for cell replacement therapy and tissue regeneration. An easily accessible cell source, the placenta, allows us to potentially establish a bio-bank of cells for immunotype matched clinical applications. Several xeno-free (XF) cryopreservation media are currently available for pluripotent stem cells, however, these media have not yet been evaluated for the cryopreservation of amnion-derived stem cells.

Methods

Human amniotic epithelial cells were collected using standard protocols, and stored at −160 °C in one of five commercially available media. Cells frozen in standard media containing fetal bovine serum served as controls. Cells were then thawed, and evaluated for viability, mitochondrial membrane stability, and senescence status. Quantitative real time PCR was utilized to assess for expression of stem cell genes, and flow cytometry was used to identify the stem cell surface markers.

Results

Cell recovery and repopulation assays indicated no significant difference between XF media versus standard cryopreservation medium. In addition, no impact was observed on the senescence status, the cytostructural or mitochondrial morphology between the tested cryopreservation media. Differences were observed on the expression of stem cell marker genes (OCT4, SOX2, and NANOG) and a cell surface marker (TRA1-60) following cryopreservation in different chemically defined XF media, however, these were not statistically significant.

Conclusions

Xeno-free cryopreservation of human amnion-derived stem cells is feasible and can be standardized to establish a bio-bank with human amnion-derived stem cells for future clinical application. Optimization of this media may allow for improved preservation of stem cell-like characteristics.

Keywords

Placenta Amniotic epithelial cells Placenta-derived stem cells Cryopreservation Serum-free Xeno-free Chemically defined media

Background

Over the last decade, there has been a growing interest in the placenta as a rich source of stem cells [1, 2] without the limitations and ethical concerns associated with the use of other pluripotent stem cell sources. Human amniotic epithelial cells (hAECs) are derived from the epiblast and retain stem cell-like characteristics [3, 4]. Although pluripotency of a single amniotic epithelial (AE) cell has not yet been identified, under appropriate culture conditions hAECs exhibit the capability of differentiating into all three germ layers [5, 6]. A variety of preclinical studies have already shown the promising therapeutic value of hAECs [712]. The large volume of available placental tissue in conjunction with limited ethical concerns of the cell source, suggests the possibility of a biobank system to provide immunotype-matched hAECs for future clinical applications [13].

It is essential to establish a reliable and reproducible cryopreservation protocol for a clinically applicable biobanking system. Ideally, the banking system would be networked among multiple procurement centers to provide all needed immunotypes [14]. In order to establish the multicenter network, the cryopreservation protocol needs to be standardized to maintain homogeneity of banked cells, and allow them to maintain their stem cell-like characteristics. This concept has already been applied to the cryopreservation of hematopoietic stem cells for clinical applications [12, 15]. The cryopreservation protocols for other emerging progenitor cell populations have also been demonstrated in several studies [1619], however, it has not been demonstrated for hAECs.

Conventional cryopreservation media contains fetal bovine serum (FBS), a mixture of growth factors, cytokines and undefined substances which includes bovine exosomes [2022]. These undefined substances, and the concern for transmission of zoonotic disease, prohibit the use of FBS when establishing a standardized cryopreservation protocol for clinical use in humans. Several serum-free cryopreservation media and methods have been developed and distributed on the market as good manufacturing practice (GMP)-compliant or GMP-amenable products [15, 2325]. The aim of this study is to demonstrate the feasibility in establishing a standardized cryopreservation protocol with commercially available, xeno-free, chemically defined cryopreservation medium for future clinical therapy.

Methods

Isolation and culture of human amniotic epithelial cells

Human placentae were obtained from the Los Angeles County and University of Southern California Medical Center. All placental samples were de-identified and otherwise considered medical waste. The tissue collection was approved as non-human subject (45 CFR 46.102(f)), which does not require consent, by the University of Southern California Health Sciences institutional review board (IRB: HS-11-00206). Only those from healthy mothers undergoing uncomplicated elective caesarean deliveries were utilized. Any patient testing positive for human immunodeficiency virus, hepatitis B virus, hepatitis C virus, tuberculosis, chlamydia trachomatis, neisseria gonorrhoeae, syphilis or any placenta showing any macroscopic abnormality were excluded. hAECs were enzymatically isolated from the amniotic membrane as previously described [26].

In brief, the amnion layer was mechanically separated from the chorion layer and washed several times with phosphate-buffered saline without calcium and magnesium (PBS) to remove blood. To dissociate AE cells, the amniotic membrane was incubated at 37 °C with 0.05 % trypsin containing 0.53 mM EDTA4Na (Life Technologies, Grand Island, NY, USA). Digesta from the first 10 minutes of the trypsin digestion were discarded to exclude debris. Cells from the second and third 40-minute digests were pooled and washed three times with PBS. The viability of the AE cells was determined by exclusion of trypan blue dye and counted with a hemocytometer. Cells were cultured at 65 × 103/cm2 in high-glucose DMEM with 10 % FBS supplemented 10 ng/ml recombinant human epidermal growth factor (AF-100-15, PEPROTECH, Rocky Hill, NJ, USA). Unattached cells and debris were removed after 24 h. One million cells were used immediately for characterization as a day-0 sample. After culturing for 5 days, cells were dissociated with trypsin and cryopreserved as described below.

Cryopreservation and thawing procedures

Five commercial xeno-free cryopreservation media were examined: CryoStor CS10, CryoStor CS5 (BioLife Solutions, Bothell, WA, USA), STEM-CELLBANKER (amsbio, Cambridge, MA, USA), CryoStem (Stemgent, Lexington, MA, USA), and Synth-a-Freeze (Life Technologies) (Table 1). Standard cryomedium (FBS-10: 90 % FBS + 10 % dimethyl sulfoxide (DMSO)) was used as a control. Cells were washed twice with PBS and resuspended at a concentration of 1 × 106 cells/ml in each ice-cooled cryomedium, and transferred to cryotube vials (Nunc Cryotube, Thermo Scientific, Waltham, MA, USA) samples were cooled in a standard freezing container (Nalgene, Thermo Scientific) to −80 °C at −1 °C/min. After 24 h, samples were transferred to a liquid nitrogen tank and cryopreserved for 2 weeks at the vapor phase of liquid nitrogen (−151 to approximately −172 °C). To thaw cryopreserved samples, cryotubes were placed in a 37 °C water bath for rapid thawing until almost no ice was detectable. Cell viability was examined immediately after thawing, using the trypan blue exclusion method. Cells were washed once with culture medium and cultured in triplicate on 6-well culture plates, 4-chamber slides for chemifluorescence analyses, or 96-well plates for (3-(4,5-dimethyl-2-thiazolyl)-2,5-diphenyl-2H-tetrazolium bromide (MTT) assay at 37 °C, 5 % CO2 incubator.
Table 1

Tested cryopreservation media

Medium

Brand name

Provider

Cat number

1

CryoStor CS10

BioLife Solutions

210102

2

CryoStor CS5

BioLife Solutions

205102

3

STEM-CELLBANKER

amsbio

11897

4

CryoStem

Stemgent

01-0013-51

5

Synth-a-Freeze

Life Technologies

A12542-01

Commercially available xeno-free cryopreservation media used for this study

Determination of cell viability and recovery

The impact of cryomedia on the cell repopulation cell viability was tested by MTT assay. Briefly, the AE cells (104 cells/well) were plated into flat bottom 96-well tissue culture plates. After 48 h, 10 ul MTT solution (Biotium, Hayward, CA, USA) was added to 100 ul of medium in each well. The plates were incubated at 37 °C for 2 h. The 570 nm absorbance and 630 nm background signal was measured and subsequently subtracted from the signal absorbance to calculate a normalized absorbance value. Cell repopulation was defined by the MTT assay as the amount of viable cells repopulated following cryopreservation, and cell recovery was defined as the percentage of viable cells following cryopreservation as compared to the number of pre-freeze viable cells.

Chemifluorescence analysis

To examine the effects of freezing on mitochondrial membrane stability, MitoTracker Red CMXRos (Life Technologies) was used to visualize the mitochondria of hAECs following the manufacturer’s instructions. Briefly, after thawing, hAECs were cultured on a permanox 4-chamber slide (Lab-Tek, Thermo Fisher Scientific) for 2 days. When cultures reached 50 % confluency, hAECs were permeabilized by immersion in 0.1 % Triton X-100 in PBS for 10 minutes and incubated in AE media containing 2 nM of Mitotracker Red CMXRos for 25 minutes. Cells were then washed twice with PBS and fixed in 2 % (w/v) paraformaldehyde in PBS. To examine the cell membrane and cytoskeleton integrity, cells were simultaneously stained with Alexa Fluor 488 conjugated phalloidin (1:40, Life Technologies). 4′,6-diamidino-2-phenylindole (DAPI) containing mountant (ProLong Gold Antifade Mountant, Life Technologies) was used to seal the slides and counterstain nuclei. The stained hAEC images were captured using either a LSM 5 Exciter confocal laser-scanning microscope or an Axiovert 200 fluorescence/live cell imaging microscope (ZEISS, Thornwood, NY, USA). The CMXRos fluorescence intensity was analyzed with a scientific image-analysis program, ImageJ. The chemifluorescent images were split to three RGB channels, with the blue channel images used to count the number of nuclei and the red channel images for quantification of the integrated density of CMXRos.

Real-time quantitative PCR

Total RNA was isolated utilizing the RNeasy Plus Mini Kit (Qiagen, Valencia, CA, USA) following the manufacturer’s protocol and the cDNA was synthesized from 1 μg RNA using qScript™ cDNA SuperMix (Quanta Biosciences, Gaithersburg, MD, USA). Quantitative real-time PCR (qRT-PCR) was carried out using the ViiA™ 7 Real-Time PCR System (Life Technologies) with PerfeCTa SYBR Green SuperMix (Low ROX) master mix (Quanta Biosciences). All reactions were carried out on the same plate in duplicate with amplification of the target genes: POU domain class 5 transcription factor 1 (OCT4), SRY (sex determining region Y)-box 2 (SOX2), Nanog homeobox (NANOG), alpha-L-iduronidase (IDUA), branched chain keto acid dehydrogenase E1, alpha polypeptide (BCKDHa), and the endogenous housekeeping gene, peptidylprolyl isomerase A (PPIA). Relative quantitative evaluation of target genes was determined by comparative cycle threshold (Ct) method (2–(delta)(delta)Ct method). The delta-Ct value from the FBS-10 group was used as the biological reference value. Primer sequences were hOCT4A-F 5′-ctt cgc aag ccc tca ttt c-3′, hOCT4A-R 5′-gag aag gcg aaa tcc gaa g-3′, Sox2-F 5′-tgc tgc ctc ttt aag act agg ac-3′, Sox2-R 5′-cct ggg gct caa act tct ct-3′, NANOG-F 5′-aga tgc ctc aca cgg aga ct-3′, NANOG-R 5′-ttt gcg aca ctc ttc tct gc-3′, IDUA-F 5′-tgg agg agc aca ggc ttc-3′, IDUA-R 5′-cca gct gag gac gta ctg gt-3′, BCKDHa-F 5′- gac ctg gtg ttt ggc cag ta-3′, BCKDHa-R 5′- tgg gcc atg aat agt tcc ag-3′, PPIA-F 5′-cct aaa gca tac ggg tcc tg-3′, PPIA-R 5′-ttt cac ttt gcc aaa cac ca-3′.

Flow cytometric analysis

Samples were prepared with 1 × 106 cells in 100 ul PBS with 1 % FBS and incubated for 40 minutes at 4 °C with the following antibodies; fluorescein isothiocyanate (FITC) conjugated Anti-TRA-1-60 antibody (mouse IgM, FCMAB115F, Millipore, Billerica, MA, USA), FITC conjugated Anti-Human Embryonic Stem Cell Antigen-1 (HESCA-1) antibody (mouse IgM, FCMAB111F, Millipore) and FITC conjugated isotype mouse IgM (clone:11E10, eBioscience, San Diego, CA, USA). After incubation, cells were washed and analyzed with the BD LSR II Analyzer and BD FACSDiVaTM Software Version 6.1 (BD Biosciences, San Jose, CA, USA), or FlowJo 10.0.8 data analysis software (FLOWJO LLC, Ashland, OR, USA).

Senescence detection assay

Cryopreserved hAECs were tested for senescence with the use of the cellular senescence detection kit (Biovision, Mountain View, CA, USA), which histochemically detects senescence-associated lysosomal β-galactosidase (SA-β-Gal) expression. After 2 weeks of cryopreservation in cryopreservation media, hAEC were maintained in the standard medium at 37 °C in 5 % CO2 for 21 days with three passages. Prior to the senescence detection assay, cells were seeded in 12-well plates at a density of 105 cells/well. The hAECs were subsequently fixed and stained for 18 h at 37 °C according to manufacturer’s instructions. Five phase contrast images were randomly acquired from one well at × 10 magnification. The number of SA-β-Gal positive cells were counted and the ratio of senescent cells/total number of nuclear was calculated.

Statistical analysis

Results are expressed as mean ± standard error of the mean (SEM). To minimize the influence of the variability of clinical samples, we normalized the data with FBS-10 data for each case and expressed as relative values. Statistical analysis was performed with Prism 5.0a (GraphPad Software, San Diego, CA, USA). Experimental and control groups were compared with paired or unpaired one-way analysis of variance (ANOVA) with Bonferroni post hoc analysis and Dunnett’s multiple comparison test. A value of p <0.05 was considered statistically significant.

Results

Impact of serum and xeno-free cryopreservation media on human amniotic epithelial cells

A total of 18 human placentae were obtained to isolate hAECs. Two of them were excluded from the study due to the low cell attachment at the time of initial plating. In the remaining 16 cases, more than 70 % of isolated the hAECs attached to uncoated cell culture-grade dishes and demonstrated the typical cobblestone shape morphology under epidermal growth factor (EGF) supplementation as described previously [5]. The hAECs proliferated and reached about 80 % confluence on day 5 after isolation. Five commercial xeno-free cryomedia, proposed for stem cell cryopreservation, were selected; CryoStor CS10, CryoStor CS5 (BioLife), STEM-CELLBANKER (amsbio), CryoStem (Stemgent), and Synth-a-Freeze (Life Technologies) and were compared with a standard cryomedium (FBS-10: 90 % FBS + 10 % DMSO). All of these cryomedia contain 5 to approximately 15 % DMSO. The impacts of each xeno-free cryopreservation medium on post-thaw cell recovery and cell repopulation were evaluated (n = 12). The absolute number of viable cells in each tube was directly counted after cryopreservation by the trypan blue exclusion method utilizing a hemocytometer (Fig. 1a). The cell repopulation capability was evaluated 48 h after thawing by using a quantitative colorimetric MTT assay (Fig. 1b). After cryopreservation, no significant differences were observed in either cell viability or cell repopulation capability between the different cryopreservation media.
Fig. 1

Comparison of cell recovery and repopulation capability. Cell viability was analyzed immediately after thawing, using the trypan blue exclusion method (n = 12). The mean value with standard error of the mean (SEM) of each group is presented (a). Cell repopulation capability after cryopreservation was evaluated 48 h after thawing, using the MTT assay (n = 12). The absorbance (A570–A630) values were normalized to unfrozen (Live) sample values. The percentage ratio with SEM of each group is presented (b)

Confocal microscopic analysis of cell membrane integrity and mitochondria damage after cryopreservation

Confocal microscopic fluorescent images illustrate the actin cytoskeleton and mitochondria quality after cryopreservation with each tested medium (Fig. 2a). Cells isolated from eight different placentae were examined. Two days after thawing, cells were stained with Mitotracker Red Chloromethyl-X-rosamine (CMXRos) and counterstained with Alexa488 conjugated phalloidin and DAPI. CMXRos is a lipophilic cationic fluorescent dye that is concentrated inside mitochondria. As this localization is dependent on the mitochondrial membrane potential, the fluorescence intensity represents the overall mitochondrial membrane potential of the cells. We have evaluated the CMXRos fluorescence intensity in each cryopreservation media exposed sample using a scientific image-analysis program, ImageJ (n = 8). The chemifluorescent images were split into three RGB channels; blue channel images were used to count the number of nuclei and red channel images were used to measure the integrated density of CMXRos. Each integrated density value was normalized by the number of nuclei to obtain an arbitrary number of CMXRos intensity per cell. The average and SEM values were plotted as relative to the value of FBS standard cryopreserved samples (Fig. 2b). CMXRos fluorescence intensity per cell was slightly higher in the CELL BANKER-treated cells, however these differences were not statistically significantindicating that all tested cryomedia preserved the mitochondrial membrane potential of these cells. There was no observable difference in cytoplasmic loss or mitochondrial clustering in any of the groups. Most cells revealed typical epithelial cell morphology on the uncoated permanox surface within a size of up to 30 μm. Some cells were small and round in shape (about 10 μm in diameter). Based on previously reported observations the small cells were expected to be undifferentiated or immature cells, which may retain stem cell-like characteristics [5]. There were no significant differences between the samples in the number of small cell populations (Fig. 2c).
Fig. 2

Cell and mitochondria morphology. Cell and mitochondria morphology was evaluated by chemifluorescence 2 days after thawing (n=8). The cells were stained with Alexa Fluor 488-phalloidin (green) to visualize actin filaments and MitoTracker Red (LifeTech, M7512) to evaluate mitochondria membrane stability (a). We used 4′,6-diamidino-2-phenylindole to counterstain the cell nuclei (blue). Scale bars represent 20 μm. CMXRos fluorescence intensity was measured with ImageJ and the average and standard error of the mean (SEM) were plotted as relative to the value of FBS control group (b). Numbers of small round cells were counted with ImageJ software and mean number of cells per mm2 of each group is presented with SEM (c).

Stem cell characteristics of hAEC after preservation

The expression of the stem cell marker genes (n = 12; OCT4, SOX2 and NANOG) and the stem cell surface markers (n = 6; TRA1-60 and HESCA-1) was examined after cryopreservation. Cells cryopreserved with STEM-CELLBANKER best preserved expression of the stem cell marker genes (Fig. 3a). Significant differences were not detected between groups using one-way ANOVA; OCT4 (p = 0.4513), SOX2 (p = 0.6686), and NANOG (p = 0.2088). However, the relative expression of all stem cell marker genes in cells cryopreserved in STEM-CELLBANKER and CryoStem were increased as compared to the other three cryomedia. No differences were detected in expression of the functional enzyme genes, IDUA and BCKDHa, in cells preserved in the different media (Fig. 3b).
Fig. 3

Stem cell marker genes expression. Real-time quantitative PCR analyses reveal relative stem cell marker gene (a) and functional enzyme gene (b) expression after cryopreservation (n = 12). Levels of gene expression were plotted against conventional FBS/10 % dimethyl sulfoxide (DMSO) cryopreservation medium

Flow cytometric analyses were performed to examine the embryonic stem cell surface markers, TRA1-60 and HESCA-1 (n = 6). The forward scatter (FSC) and side scatter (SSC) gating revealed the hAEC to be a single cell population in cell size and complexity. Subsequently, the FSC-H and FSC-A gating was applied to identify single cell events. The ratio of stem cell surface marker positive cells was determined with the FITC intensity and FSC-A gating (Fig. 4a). Overall both stem cell markers were expressed in approximately 5 % of cryopreserved hAEC, however, this expression was varied in each placenta. In order to demonstrate the impact of different cryopreservation media, the relative value of each group as compared to FBS samples was calculated and analyzed with one-way ANOVA using Dunnet’s multiple comparison test (n = 6). Although STEM-CELL BANKER and Synth-a Freeze cryomedia relatively preserved more tumor rejection antigen (TRA)1–60-positive cells than other cryomedia, these differences were not significant (p = 0.2596). Nor was there a difference between the groups in the number of human embryonic stem cell antigen-1 (HESCA-1)-positive cells (p = 0.3680) (Fig. 4b).
Fig. 4

Stem cell surface marker expression. Representative pseudo-color density plots demonstrate gating strategy in flow cytometric analyses (a). The relative value of tumor rejection antigen (TRA) 1–60 and human embryonic stem cell antigen-1 (HESCA-1)-positive cells to control samples was plotted for the comparison of each xeno-free cryopreservation medium (b). AE amniotic epithelial, SSC side scatter, FSC forward scatter

Fig. 5

Post-cryopreservation senescence marker activity. Cryopreserved human amniotic epithelial cells were cultured for 21 days and the influence of cryopreservation was evaluated by senescence-associated-beta-galactosidase (SA-βgal) activity, which is detectable in the cytoplasmic blue color staining (a). The ratio of SA-β-Gal-positive cells was calculated and demonstrated as mean ± standard error of the mean (b)

Senescence-associated lysosomal β-galactosidase activity in crypreserved hAECs

The ratio of senescence-associated lysosomal β-galactosidase (SA-β-Gal)-positive cells was not significantly different between the tested cryomedia (p = 0.7677, one-way ANOVA). In the FBS/DMSO control group 37.15 ± 3.601 % of hAEC were positive for SA-β-Gal, whereas other groups with xeno-free media preserved the following results were observed; CryoStor CS10: 47.22 ± 6.497 %, CryoStor CS5: 49.18 ± 5.081 %, STEM-CELL BANKER: 49.15 ± 8.118 %, CryoStem: 50.00 ± 6.951 %, and Synth-a-Freeze: 48.11 ± 6.588 % (Fig. 5). Consistent with the cell recovery and repopulation capability data, no impact of xeno-free cryomedia was observed and there was no significant difference between the tested xeno-free cryomedia.

Discussion

The establishment of an efficient and simple cryopreservation protocol is crucial for a consistent supply of a sufficient number of cells for future clinical applications, as human pluripotent stem cells are known to be highly susceptible to freeze-thaw damage. Vitrification techniques have been used to improve the recovery of stem cells; however, the procedure is cumbersome and the high osmolality of the cryopreservation media are highly toxic to the cells. In this current study we have successfully applied commercially available serum-free and xeno-free chemically defined media to cryopreserve hAECs with a simple slow freezing protocol. Conventional slow freezing media contain 5–20 % DMSO and/or glycerol as cryoprotectants to prevent formation of micro ice crystals, which impair cytoplasmic structures including the cytoskeleton fibers [27, 28] and the mitochondrial membrane [2932]. Traditional freezing medium also contains high concentrations of FBS, which increases not only the risks of undesired immunological reactions but also zoonosis. Over the last decade alternative cryoprotective substances, which avoid these potential problems have been developed, including disaccharide trehalose [33], oligosaccharide [34], and sericin [35]. These allow for the cryopreservation and recovery of human pluripotent stem cells without the loss of stem cell characteristics [36]. Among these newly developed cryopreservation media, we tested five different commercially available xeno-free chemically defined freezing media with a simple in-suspension slow freezing protocol. All five freezing media successfully cryopreserved human AE cells, and allowed for their recovery. We were able to visualize the linear polymer microfilaments, filamentous actin (F-actin), with fluorescein-conjugated phalloidin, and no differences were seen in the cytoskeletal morphology between hAECs preserved in the different media. Similarly, following cell staining with Mitotracker Red CMWRos, no differences were seen between the cryomedia in the effect on mitochondrial membrane stability.

Differences were observed between tested media in the preservation of both stem cell surface antigens and marker genes. Of the commercially available cryopreservation media tested, STEM CELL BANKER, appeared superior in preserving the pluripotent stem cell marker genes; OCT4, SOX2 and NANOG, and the stem cell surface markers TRA1–60, however, this difference was not statistically significant. Our study further supports existing data showing the high cryopreservation efficiency of STEM CELL BANKER cryomedia, previously demonstrated in mouse induced pluripotent stem (iPS) cells [17], human iPS cells [37, 38], mesenchymal stem cells [39], and primary hepatocytes [40]. None of these studies compared these media with other commercially available xeno-free chemically defined freezing media or examined the effect of these media on transcription and expression of stem cell markers.

To the best of our knowledge, this is the first report to demonstrate that STEM CELL BANKER cryomedia preserves stem cell populations of primary hAECs and, when compared to other commercially available media, allows for improved maintenance of stem cell characteristics. Scanning electron microscopy would be useful in order to further analyze membrane integrity and structural alterations. It is unlikely however, that the impact on membrane integrity and structural alterations would influence only stem cell characteristics and not cell recovery and viability. It has been disclosed that STEM CELLBANKER contains 10 % DMSO, glucose, and high molecular weight polymer in PBS [37]. Due to the proprietary information on the exact contents of the media, further mechanism analysis on the preservation of stem cell characteristics is limited.

Two major advantages of using commercially available cryopreservation media are the availability and the quality. Both parameters are essential to establish a standardizing protocol, which can be applied to isolate hAECs in a wide range of otherwise non-standard conditions. Unlike other stem cells, amnion-derived stem cells can be isolated from human placentae, which are normally discarded as medical waste and therefore readily available in most countries. To establish an efficient biobank system, networking the cell supply with the standardized isolation/cryopreservation protocol is essential. A quality-controlled product is currently most suitable for this purpose. As mentioned above the STEM CELLBANKER media has already been utilized with various human cell types currently in consideration for clinical applications and thus, there are accumulating safety data for its use in clinical trials. In addition to providing consistent materials for use in any standardized protocol, this will allow for a more streamlined clearance of regulatory hurdles for its use with alternative cell sources. Taken together, commercially available cryopreservation media are good candidates for further investigation when establishing standardized cryopreservation protocols.

Conclusions

In conclusion, the current study demonstrates that all tested commercially available xeno-free cryopreservation media successfully cryopreserved human amniotic epithelial cells without losing post-thaw cell viability and repopulation ability. Variable results were observed between the tested cryopreservation media in the preservation of stem cell characteristics of human amnion-derived stem cells. Although STEM CELLBANKER appeared to best maintain the stem cell markers in hAECs, the differences were not statistically significant. A larger sample size might better discern this. These data indicate that establishing a standardized cryopreservation protocol using commercially available xeno-free media is feasible for amnion-derived stem cell banking.

Abbreviations

AE: 

amniotic epithelial

ANOVA: 

analysis of variance

BCKDHa: 

branched chain keto acid dehydrogenase E1, alpha polypeptide

Ct: 

cycle threshold

DAPI: 

4′,6-diamidino-2-phenylindole

DMEM: 

Dulbecco’s modified Eagle’s medium

DMSO: 

dimethyl sulfoxide

ES: 

embryonic stem

FBS: 

fetal bovine serum

FITC: 

fluorescein isothiocyanate

FSC: 

forward scatter

GMP: 

good manufacturing practice

hAEC: 

human amniotic epithelial cell

IDUA: 

alpha-L-iduronidase

iPS: 

induced pluripotent stem

MTT: 

(3-(4,5-dimethyl-2-thiazolyl)-2,5-diphenyl-2H-tetrazolium bromide

NANOG: 

nanog homeobox

OCT-4: 

POU domain, class 5, transcription factor 1

PBS: 

phosphate-buffered saline

PPIA: 

peptidylprolyl isomerase A

SA-β-Gal: 

senescence-associated lysosomal β-galactosidase

SEM: 

standard error of the mean

SOX-2: 

SRY- sex determining region Y-box 2

SSC: 

side scatter

SSEA: 

stage-specific embryonic antigen

TRA: 

tumor rejection antigen

Declarations

Acknowledgements

WW and EZ were supported by the USC Science, Technology And Research (STAR) program. The authors appreciate Dr. Roberta Diaz Brinton and Ms. Glendy Ramirez-De La Cruz for directing and coordinating the program. The authors would like to thank Ms. Lora Barsky and Ms. Bernadette Masinsin for their excellent technical assistance on flow cytometric analysis. This work was supported by California Institute for Regenerative Medicine (CIRM) grant TR3-05488 (TM).

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.

Authors’ Affiliations

(1)
Department of Biochemistry and Molecular Biology, Keck School of Medicine, University of Southern California
(2)
Department of Obstetrics and Gynecology, Keck School of Medicine, University of Southern California
(3)
Eli and Edythe Broad Center for Regenerative Medicine and Stem Cell Research at USC, Keck School of Medicine, University of Southern California

References

  1. Parolini O, Alviano F, Bagnara GP, Bilic G, Bühring H-J, Evangelista M, et al. Concise review: isolation and characterization of cells from human term placenta: outcome of the first international Workshop on Placenta Derived Stem Cells. Stem Cells. 2008;26:300–11.PubMedView ArticleGoogle Scholar
  2. Ilancheran S, Moodley Y, Manuelpillai U. Human Fetal Membranes: A Source of Stem Cells for Tissue Regeneration and Repair? Placenta. 2009;30:2–10.PubMedView ArticleGoogle Scholar
  3. Miki T. Amnion-derived stem cells: in quest of clinical applications. Stem Cell Res Ther. 2011;2:25.PubMedPubMed CentralView ArticleGoogle Scholar
  4. Miki T, Grubbs B. Therapeutic potential of placenta-derived stem cells for liver diseases: Current status and perspectives. J Obstet Gynaecol Res. 2014;40:360–8.PubMedView ArticleGoogle Scholar
  5. Miki T, Lehmann T, Cai H, Stolz DB, Strom SC. Stem cell characteristics of amniotic epithelial cells. Stem Cells. 2005;23:1549–59.PubMedView ArticleGoogle Scholar
  6. Ilancheran S, Michalska A, Peh G, Wallace EM, Pera M, Manuelpillai U. Stem cells derived from human fetal membranes display multilineage differentiation potential. Biol Reprod. 2007;77:577–88.PubMedView ArticleGoogle Scholar
  7. Manuelpillai U, Lourensz D, Vaghjiani V, Tchongue J, Lacey D, Tee J-Y, et al. Human amniotic epithelial cell transplantation induces markers of alternative macrophage activation and reduces established hepatic fibrosis. PLoS One. 2012;7, e38631.PubMedPubMed CentralView ArticleGoogle Scholar
  8. Skvorak KJ, Dorko K, Marongiu F, Tahan V, Hansel MC, Gramignoli R, et al. Placental stem cell correction of murine intermediate maple syrup urine disease. Hepatology. 2013;57:1017–23.PubMedPubMed CentralView ArticleGoogle Scholar
  9. Liu YH, Vaghjiani V, Tee JY, To K, Cui P, Oh DY, et al. Amniotic epithelial cells from the human placenta potently suppress a mouse model of multiple sclerosis. PLoS One. 2012;7, e35758.PubMedPubMed CentralView ArticleGoogle Scholar
  10. Moodley Y, Vaghjiani V, Chan J, Baltic S, Ryan M, Tchongue J, et al. Anti-inflammatory effects of adult stem cells in sustained lung injury: a comparative study. PLoS One. 2013;8, e69299.PubMedPubMed CentralView ArticleGoogle Scholar
  11. Toda A, Okabe M, Yoshida T, Nikaido T. The potential of amniotic membrane/amnion-derived cells for regeneration of various tissues. J Pharmacol Sci. 2007;105:215–28.PubMedView ArticleGoogle Scholar
  12. Parolini O, Alviano F, Bergwerf I, Boraschi D, De Bari C, De Waele P, et al. Toward cell therapy using placenta-derived cells: disease mechanisms, cell biology, preclinical studies, and regulatory aspects at the round table. Stem Cells Dev. 2010;19:143–54.PubMedView ArticleGoogle Scholar
  13. Strom SC, Skvorak K, Gramignoli R, Marongiu F, Miki T. Translation of amnion stem cells to the clinic. Stem Cells Dev. 2013;22 Suppl 1:96–102.PubMedView ArticleGoogle Scholar
  14. Nakatsuji N, Nakajima F, Tokunaga K. HLA-haplotype banking and iPS cells. Nat Biotechnol. 2008;26:739–40.PubMedView ArticleGoogle Scholar
  15. Massie I, Selden C, Hodgson H, Fuller B, Gibbons S, Morris GJ. GMP Cryopreservation of large volumes of cells for regenerative medicine: active control of the freezing process. Tissue Eng Part C Methods. 2014;20:1–46.View ArticleGoogle Scholar
  16. Roy S, Arora S, Kumari P, Ta M. A simple and serum-free protocol for cryopreservation of human umbilical cord as source of Wharton’s jelly mesenchymal stem cells. Cryobiology. 2014;68:467–72.PubMedView ArticleGoogle Scholar
  17. Miyamoto Y, Noguchi H, Yukawa H, Oishi K, Matsushita K, Iwata H, et al. Cryopreservation of induced pluripotent stem cells. Cell Med. 2012;3:89–95.View ArticleGoogle Scholar
  18. Cohen RI, Thompson ML, Schryver B, Ehrhardt RO. Standardized cryopreservation of pluripotent stem cells. Curr Protoc Stem Cell Biol. 2014;28:Unit 1C.14.PubMedGoogle Scholar
  19. Jorns C, Ellis EC, Nowak G, Fischler B, Nemeth A, Strom SC, et al. Hepatocyte transplantation for inherited metabolic diseases of the liver. J Intern Med. 2012;272:201–23.PubMedView ArticleGoogle Scholar
  20. Gook DA, Edgar DH. Human oocyte cryopreservation. Hum Reprod Update. 2007;13:591–605.PubMedView ArticleGoogle Scholar
  21. Li Y, Tan J-C, Li L-S. Comparison of three methods for cryopreservation of human embryonic stem cells. Fertil Steril. 2010;93:999–1005.PubMedView ArticleGoogle Scholar
  22. Karlsson JOM, Toner M. Long-term storage of tissues by cryopreservation: Critical issues. Biomaterials. 1996;17:243–56.PubMedView ArticleGoogle Scholar
  23. Mitry RR, Lehec SC, Hughes RD. Cryopreservation of human hepatocytes for clinical use. Methods Mol Biol. 2010;640:107–13.PubMedView ArticleGoogle Scholar
  24. Polchow B, Kebbel K, Schmiedeknecht G, Reichardt A, Henrich W, Hetzer R, et al. Cryopreservation of human vascular umbilical cord cells under good manufacturing practice conditions for future cell banks. J Transl Med. 2012;10:98.PubMedPubMed CentralView ArticleGoogle Scholar
  25. Stacy GN, Masters JR. Cryopreservation and banking of mammalian cell lines. Nat Protoc. 2008;3:1981–89.View ArticleGoogle Scholar
  26. Miki T, Marongiu F, Dorko K, Ellis ECS, Strom SC. Isolation of amniotic epithelial stem cells. Curr Protoc Stem Cell Biol. 2010;Chapter 1:Unit 1E.3.PubMedGoogle Scholar
  27. Hall SM, Evans J, Haworth SG. Influence of cold preservation on the cytoskeleton of cultured pulmonary arterial endothelial cells. Am J Respir Cell Mol Biol. 1993;9:106–14.PubMedView ArticleGoogle Scholar
  28. Ahn HJ, Sohn IP, Kwon HC, Jo DH, Park YD, Min CK. Characteristics of the cell membrane fluidity, actin fibers, and mitochondrial dysfunctions of frozen-thawed two-cell mouse embryos. Mol Reprod Dev. 2002;61:466–76.PubMedView ArticleGoogle Scholar
  29. Wilson JM, Caceci T, Potter GD, Kraemer DC. Ultrastructure of cryopreserved horse embryos. J Reprod Fertil Suppl. 1987;35:405–17.PubMedGoogle Scholar
  30. Sammut IA, Thorniley MS, Simpkin S, Fuller BJ, Bates TE, Green CJ. Impairment of hepatic mitochondrial respiratory function following storage and orthotopic transplantation of rat livers. Cryobiology. 1998;36:49–60.PubMedView ArticleGoogle Scholar
  31. Ogier de Baulny B, Labbé C, Maisse G. Membrane integrity, mitochondrial activity, ATP content, and motility of the European catfish (Silurus glanis) testicular spermatozoa after freezing with different cryoprotectants. Cryobiology. 1999;39:177–84.PubMedView ArticleGoogle Scholar
  32. Stéphenne X, Najimi M, Ngoc DK, Smets F, Hue L, Guigas B, et al. Cryopreservation of human hepatocytes alters the mitochondrial respiratory chain complex 1. Cell Transplant. 2007;16:409–19.PubMedView ArticleGoogle Scholar
  33. Eroglu A, Russo MJ, Bieganski R, Fowler A, Cheley S, Bayley H, et al. Intracellular trehalose improves the survival of cryopreserved mammalian cells. Nat Biotechnol. 2000;18:163–7.PubMedView ArticleGoogle Scholar
  34. Miyamoto Y, Suzuki S, Nomura K, Enosawa S. Improvement of hepatocyte viability after cryopreservation by supplementation of long-chain oligosaccharide in the freezing medium in rats and humans. Cell Transplant. 2006;15:911–9.PubMedView ArticleGoogle Scholar
  35. Miyamoto Y, Teramoto N, Hayashi S, Enosawa S. An improvement in the attaching capability of cryopreserved human hepatocytes by a proteinaceous high molecule, sericin, in the serum-free solution. Cell Transplant. 2010;19:701–6.PubMedView ArticleGoogle Scholar
  36. Unger C, Skottman H, Blomberg P, Sirac dilber M, Hovatta O. Good manufacturing practice and clinical-grade human embryonic stem cell lines. Hum Mol Genet. 2008;17:R48–53.PubMedView ArticleGoogle Scholar
  37. Holm F, Ström S, Inzunza J, Baker D, Strömberg A-M, Rozell B, et al. An effective serum- and xeno-free chemically defined freezing procedure for human embryonic and induced pluripotent stem cells. Hum Reprod. 2010;25:1271–9.PubMedPubMed CentralView ArticleGoogle Scholar
  38. 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. 2014;4:3594.PubMedPubMed CentralGoogle Scholar
  39. Yoshitaka M, Koichi O, Hiroshi Y, Hirofumi N, Masahiro S, Hisashi I, et al. Cryopreservation of Human Adipose Tissue-Derived Stem/Progenitor Cells. Cryobiol Cryotechnol. 2010;56:55–8.Google Scholar
  40. Saliem M, Holm F, Tengzelius RB, Jorns C, Nilsson LM, Ericzon BG, et al. Improved cryopreservation of human hepatocytes using a new xeno free cryoprotectant solution. World J Hepatol. 2012;4:176–83.PubMedPubMed CentralView ArticleGoogle Scholar

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