Patent Application
20160194609
The present invention relates to methods of isolating mesenchymal stem cells originated from Wharton's jelly (WJ-MSC) from single donor. In addition, the present disclosure also relates to sample collection media and expansion media used in these methods as well as characterization of mesenchymal stem cells and their use in the treatment of various disorders.
Stem cells (SCs) have been widely characterized as precursors that self-replicate with the ability to give rise to one or more cell types, known as potency. Stem cells can be hierarchically classified as unipotent, multipotent, pluripotent and totipotent. Unipotent stem cells can produce only one cell type (e.g. neurons), whereas multipotent ones can differentiate into several cell types (e.g. hematopoietic stem cells, HSCs). An embryonic stem cell (ESC), derived from the inner cell mass (ICM) of the embryo is pluripotent as it can differentiate into cells of three germ layers, but not into trophoblastic cells, whereas the zygote is totipotent as it produces cells of embryonic as well as extra-embryonic tissue. On the other hand, SCs also can be isolated from a variety of adult tissues sources such as bone marrow, skin, adipose tissues and many more. However, these sources pose limitations which include lack of starting material, invasive procurement procedures, tedious processing techniques and most importantly, limited proliferative capacity due to their adult origin.
Another source originating from extra-embryonic tissue is Wharton's jelly (WJ) of human umbilical cord which has gained popularity due to its non-controversial source and abundance in mesenchymal stem cells (MSC) population from its raw starting material as disclosed by McGuirk and Weiss, in Placenta, vol. 32, pages S304-10 (2011). Further, WJ-MSCs share many properties with adult mesenchymal stem cells originated from bone marrow (BM-MSCs), but are generally considered as a more primitive population than the latter. In fact, while they possess several characteristics of ESCs, they do not form teratomas upon transplantation and their research does not raise ethical or legal issues. All these features open attractive perspectives for the propagation and engineering of WJ-MSCs for cell-based therapies.
In addition, they are also relatively easy to harvest and to process as compared to bone marrow or embryonic origin prior to ex vivo expansion as testified by C. C. Yang et al, in Plos One, vol. 3, doi: 10.1371/journal.pone.0003336 (2008). Another advantage of this source is that these cells have high proliferation rates, wide multi-potency, hypo-immunogenicity, do not induce tumorigenesis and have anti-tumor properties as claimed by C. Y. Fong et al, in Stem Cell Reviews, vol. 7, pages 1 to 16 (2011).
The potential of WJ-MSC was comprehensively investigated in which exposure towards exogeneous growth factors has shown to contribute to the formation of pre-chodrocytes cells as described in U.S. Pat. No. 5,919,702 by Purchio et al. Further work to obtain enriched osteoprogenitor cells from Wharton's Jelly was conducted by Davies et al., in their U.S. Patent application 2005/0148074. Recently, Majumdar in WO2012131618 A1 has described the method of obtaining pooled WJ-MSCs for the purpose of producing an off-the-shelf product. This was meant to serve as allogeneic MSC product for therapeutics application in large scale. Though the idea is noteworthy, it should also be noted that genetic variability among donors is a confounding factor that requires serious attention.
Though the allogeneic MSC that are being used in the transplantation have been thoroughly checked for human leukocyte antigen (HLA) markers, any variation especially in terms of genetic that may occur during the course of transplantation would be very difficult to identify and subsequently control. In addition, having a pooled cell culture has another disadvantage as it might contribute to graft versus host disease in certain recipients thus requiring rigorous follow-up sessions which would be unnecessary if the cells were to have propagated from a single donor. On the other hand, among the benefits of using cells isolated from single donor are reduced disease transmission, reduced alloimmunization and superior function and storage characteristics.
Taking into consideration of all these hurdles, the present disclosure relates to a composition comprising of large scale expansion of WJ-MSC from a single donor for the purpose of allogeneic transplantation.
The present invention relates to a method of isolating mesenchymal stem cells originating from Wharton's jelly (WJ-MSC) from at least a single donor. The method for isolating and proliferating viable cells from Wharton's jelly is described herein, wherein the method includes the steps of (a) obtaining umbilical cord tissue comprising of viable cells from Wharton's jelly, (b) isolating the viable cells in a sample collection media, (c) preparing a primary stock culture using the viable cells from step (b), (d) proliferating the primary stock culture from step (c) to obtain sub-cultured stocks, (e) harvesting the viable cells from the sub-cultured stocks from step (d) and (f) cryo-preserving the viable cells from step (e) under cryogenic conditions. The present invention also discloses the sample collection media and expansion media used in the method. The present invention also discloses the characterization of the mesenchymal stem cells isolated from Wharton's jelly and their use in treating various diseases.
In view of the potential application of stem cells from Wharton's jelly for clinical medicine, there is growing interest in optimizing their expansion protocols so as to produce large quantities of cells for therapeutic applications, which is cost-effective and yet maintains their phenotype and functional capabilities. To date, there is inconsistency among laboratories concerning the isolation process example of using pooled samples. The present invention, overcomes the inconsistency by setting optimal culture conditions for effective clinical-grade production of large number of stem cells from Wharton's jelly in a short time, economizing on cost and time to serve for better cellular therapy. The results of the study are highly reproducible and consistent, making them useful for in vivo as well as in vitro manipulation without the stem cells from Wharton's jelly losing their vigour and chromosomal stability.
Upon receiving the umbilical cord from the hospital (within 48 hours post-delivery), the umbilical cord was cut into three pieces, approximately 4-5 cm long and individual segmented cord was washed three times in 30 mL of ddH2O in a 50 mL centrifuge tube to remove blood contaminant. Next, the clean cord was immersed in a 50 mL centrifuge tube containing 30 ml of Dulbecco's Phosphate Buffered Saline (DPBS), 20% Antibiotic-Antimycotic (1×) and 20% Penicillin-Streptomycin (1×). This process was repeated three times to disinfect the cord. The cord need to be stored at +4° C. until processing (within 24 hours) or can be processed immediately.
The isolation process was carried out in Biological Safety Cabinet (BSC) at a current good manufacturing practise facility with the following parameters.
Prior to the isolation process, sterilization by means of wiping the BSC surface with 70% Isopropyl Alcohol (IPA) using sterile wipes need to be done as well as UV sterilization for 30 minutes. Tubes containing the cord were transferred into the BSC. The cords were then washed three times in three different units of 50 mL centrifuge tube containing 30 mL of ddH2O, 1% Antibiotic-Antimycotic (1×) and 1% Penicillin-Streptomycin (1×) with additional heparin injection into the blood vessels to remove blood clot. By using sterile scissor (sharp/sharp), scalpel, blade and forceps, the cord was manipulated in a sterile surgical tray or culture plate. Blood vessels were then removed from each piece by incising the cord lengthwise using sterile scissor (sharp/sharp), blade and forceps. Next the cords were immersed into 70% ethanol for 30 seconds for further disinfection process before immediate immersion into ddH2O 3 times for 30 seconds per dip to completely remove the traces of 70% ethanol. The cords were transferred into new three units of 50 mL centrifuge tube containing DPBS and 5% Antibiotic-Antimycotic (1×) and incubated at 37° C. overnight. On the next day, the cords were then washed with DPBS three times with 2 minutes incubation. Each cord tissue was transferred into three new 50 mL centrifuge tubes containing 15 mL solution mixture of 4 mg/mL Collagenase Type-IV dissolved in Knockout-Dulbecco's Modified Eagle Medium (KO-DMEM). The cord tissues were later minced using sterile scissor (sharp/sharp) until it becomes tiny pieces (≈2 mm3) and incubated at 37° C. in shaking incubator for overnight.
2 mL of 0.05% Trypsin-EDTA was added the next day to the digested tissue and incubated for 10 minutes. Next, equal volume of neutralization medium containing 95% KO-DMEM and 5% FBS was added into each tube to neutralize the activity of Collagenase Type-IV. The mixture was then centrifuged at 1800 rpm for 5 minutes at room temperature (18° C.±2° C.).
Upon centrifugation, the top aqueous phase of the mixture (approximately 0.3 cm above the pale yellow phase) was slowly removed using a pipette. Further, the jelly like solution (containing dissociated cord pieces) was strained using 100 μm cell strainer into new three units of 50 mL centrifuge tube and centrifuged at 1800 rpm for 5 minutes after adding equal volume of complete culture medium (CCM)#
The supernatant was then discarded and re-suspended with 5 mL of CCM. Upon cell count, the cell suspension was cultured in three units of T25 cm2 flask at 37° C. in 5% humidified CO2 incubator and keep the flasks undisturbed for 24 hours. After 24 hours, the flasks were transferred from 5% humidified CO2 incubator to the BSC. Next the conditioned media was discarded and replaced with 5 mL of CCM before transferring them back to CO2 incubator. The cells were observed under inverted microscope every 2 days until the cells reach 80%±5% confluency. At day 7, the flasks were transferred from 5% humidified CO2 incubator to the BSC. 5 mL of CCM was added into the flask and transferred back to CO2 incubator. The same step was repeated at Day 14. Upon reaching 85%±5% confluency, cells were then sub-cultured to Subculture Cell Stock 1.
Prior to work, BSC need to be cleaned via UV sterilization for 30 minutes and also with sterile 70% Isopropyl Alcohol (IPA) and sterile wipes. The T25 cm2 culture flasks containing Subculture Cell Stock 0 (SC0) cells were transferred into cleaned and sterilized BSC. A total of 5 mL of Dulbecco's Phosphate Buffered Saline (DPBS) was used for rinsing upon removing all conditioned medium from culture flasks via serological pipettes.
The flasks were left for 1 minute and the DPBS was discarded into a waste beaker and later added with 1 mL of 0.05% Trypsin-EDTA into each flask and incubated at 37° C. in 5% humidified CO2 incubator for less than 10 minutes.
Cells were observed under inverted microscope for round and floating cells to confirm complete cell detachment. Then, Complete Culture Media (CCM) was added to neutralize 0.05% Trypsin-EDTA activity.
Cell suspension was transferred into a new 50 mL centrifuge tube and centrifuged at 1500 rpm for 10 minutes at room temperature (18° C.±2° C.). The supernatant was discarded into waste beaker and 20 mL of CCM was added into the tube to re-suspend the pellet. After performing cell count, the cells were cultured into T75 cm2 culture flasks for Subculture Cell Stock 1 (SC1) culture.
After adding up to 10 mL of CCM into the flasks, they were then incubated at 37° C. in 5% humidified CO2 incubator. The cells were observed under inverted microscope every 2 days until the cells reach 80%±5% confluency. At day 7, the flasks were transferred from 5% humidified CO2 incubator to the BSC. 5 mL of CCM was added into the flask and transferred back to CO2 incubator. The same step was repeated at Day 14. Upon reaching 85%±5% confluency, cells were then sub-cultured to Subculture Cell Stock 2.
Prior to work, BSC need to be cleaned via UV sterilization for 30 minutes and also with sterile 70% Isopropyl Alcohol (IPA) and sterile wipes. The T25 cm2 culture flasks containing Subculture Cell Stock 1 (SC1) cells were transferred into cleaned and sterilized BSC. A total of 5 mL of Dulbecco's Phosphate Buffered Saline (DPBS) was used for rinsing upon removing all conditioned medium from culture flasks via serological pipettes.
The flasks were left for 1 minute and the DPBS was discarded into a waste beaker and later added with 1 mL of 0.05% Trypsin-EDTA into each flask and incubated at 37° C. in 5% humidified CO2 incubator for less than 10 minutes.
Cells were observed under inverted microscope for round and floating cells to confirm complete cells detachment. Then, Complete Culture Media (CCM) was added to neutralize 0.05% Trypsin-EDTA activity.
Cell suspension was transferred into a new 50 mL centrifuge tube and centrifuged at 1500 rpm for 10 minutes at room temperature (18° C.±2° C.). The supernatant was discarded into waste beaker and 20 mL of CCM was added into the tube to re-suspend the pellet. After performing cell count, the cells were cultured into T75 cm2 culture flasks for Subculture Cell Stock 2 (SC2) culture.
After adding up to 10 mL of CCM into the flasks, they were then incubated at 37° C. in 5% humidified CO2 incubator. The cells were observed under inverted microscope every 2 days until the cells reach 80%±5% confluency. At day 7, the flasks were transferred from 5% humidified CO2 incubator to the BSC. 5 mL of CCM was added into the flask and transferred back to CO2 incubator. The same step was repeated at Day 14. Upon reaching 85%±5% confluency, cells were then sub-cultured to Subculture Cell Stock 2.
Prior to work, BSC need to be cleaned via UV sterilization for 30 minutes and also with sterile 70% Isopropyl Alcohol (IPA) and sterile wipes. The culture flasks containing Subculture Cell Stock 1 (SC1) cells were transferred into cleaned and sterilized BSC. Routine rinsing step was repeated twice using volume of Dulbecco's Phosphate Buffered Saline (DPBS) as shown in the table below, upon removing all conditioned medium from culture flasks via serological pipettes.
The flasks were left for 1 minute and the DPBS was discarded into a waste beaker and later added with 0.05% Trypsin-EDTA into each flask and incubated at 37° C. in 5% humidified CO2 incubator for less than 10 minutes.
Cells were observed under inverted microscope for round and floating cells to confirm complete cells detachment. Then, Complete Culture Media (CCM) was added to neutralize 0.05% Trypsin-EDTA activity.
Cell suspension was transferred into a new 250 mL centrifuge tube and centrifuged at 1800 rpm for 10 minutes at room temperature (18° C.±2° C.). The supernatant was discarded into waste beaker and 20 mL of CCM was added into the tube to re-suspend the pellet. The cells suspension was then pooled into one single 250 mL centrifuge tube. After performing cell count, the cells were then proceeded with “Retention Cells” and “Freezing Cells in Cryobag” steps. The cell suspension was split as follows:
Prior to work, BSC need to be cleaned via UV sterilization for 30 minutes and also with sterile 70% Isopropyl Alcohol (IPA) and sterile wipes. An appropriate volume of Cell Freezing Medium (CFM), with a mixture of Fetal Bovine Serum (FBS) and Dimethyl Sulfoxide (DMSO) need to be prepared at a ratio shown in the table below:
The mixture was then carefully mixed using 10 mL pipette with avoidance of bubbles formation. The tube cap needs to be tightened and wrapped with aluminium foil to protect from light. It was kept in +4° C. prior to use.
Cells from “retention cells” were centrifuged at 1500 rpm for 10 minutes at room temperature (18° C.±2° C.). The supernatant was then discarded and the pellet was re-suspended with 5 mL of the freshly prepared CFM. A total of 1 mL of CFM was transferred containing approximately 10×106 cells into each of five units labelled 1.8 mL cryogenic vials.
A 30 mL cryobag was wiped with sterile 70% IPA and transferred into the BSC. Air was fully removed to make it air-tight using a 30 mL syringe and 22 G syringe needle to avoid bubble formation during the load of the cells into the bag. Cells from ‘Freezing cells in Cryobag’ were centrifuged at 1500 rpm for 10 minutes at room temperature (18° C.±2° C.). The supernatant was then discarded and the pellet was re-suspended with 30 mL of the freshly prepared CFM. By using a 30 mL syringe, the cell suspension containing approximately 60×106 cells was loaded into a 30 mL cryobag. The cryobag was then sealed using sealer while the excess tubes were removed. Cryobags were then placed in cassettes before transferring them into −80° C. freezer for 24 to 48 hours. The cryobags were placed into a frame located in vapour phase of liquid nitrogen (LN2) storage freezer.
The proliferation rate was determined by plating 5000 cells/cm2 from WJ-MSCs and BM-MSCs (control cell lines) per T25 cm2 culture flask (BD Pharmingen, San Diego, Calif.). Three replicates were performed for each passage and time point. Cells were detached by trypsinization after reaching confluency of 90%. Cells were counted and assessed for viability by means of trypan blue dye exclusion before the next passage. Cells were replated for subsequent passages, and total of 2 passages were studied in this experiment. Growth kinetics was analysed by calculating population doubling (PD) time. The PD time was obtained using the formula:
PD=tplg2/(IgNH−IgNI),
wherein NI is the inoculum cell number, NH is the cell harvest number, and t is the time of the culture (in hours). The population doubling trend in WJMSCs is illustrated in
For Annexin V/propidium iodide (PI) assays (refer
The immunophenotyping was done by using flow cytometry at passage 2 (finish product). On reaching 90% confluency, the cells were harvested with 0.05% trypsin (Invitrogen) and resuspended in phosphate buffered saline (DPBS) at a cell density of 1.5×106 cells/mL. Two hundred microliters of the cell suspension (1×105 cells) was incubated with the labelled antibodies in the dark for 1 hour at 37° C. The following antibodies were used to mark the cell surface epitopes: CD90-phycoerythrin (PE), CD44-PE, CD73-PE, CD166-PE and CD34-PE, CD45-fluoroisothiocyanate (FITC), and HLA-DR-FITC (all from BD Pharmingen). All analyses were standardized against negative control cells incubated with isotype-specific immunoglobulin (Ig) G1-PE and IgG1-FITC (BD Pharmingen). Immunophenotyping of stem cells derived from WJSCs showed that the cells were negative for hematopoietic markers CD34 and CD45 and HLA-DR, whereas more than 90% of cells were positive for mesenchymal stem cell markers CD44, CD73, CD90, and 70.4% for CD166 (refer
The cultures were initiated at a density of 1000 cells/cm2 in 6-well plates and were grown to confluence and subjected to differentiation into adipogenic, chondrogenic, and osteogenic lineages as per the method described earlier (Pal R, Hanwate M, Jan M, et al. J Tissue Eng Regen Med 2009; 3:163-74.). Adipogenic lineage was stimulated by inducing the cells with 10% FBS, 200 mmol/L indomethacin, 0.5 mmol/L 3-isobutyl-1-methyxanthine (IBMX), 10 mg/mL insulin, and 1 mmol/L dexamethasone (all reagents from Sigma Aldrich). Lipid droplets were visualized by staining with oil red O staining (Sigma Aldrich). The percent of adipocytes was estimated by counting 500 total cells in multiple fields. The osteogenic differentiation was stimulated in a 3-week culture in media supplemented with 10% FBS, 10−7 mol/L dexamethasone, 10 mmol/L b-glycerol phosphate (Fluka, Buchs, Switzerland), and 100 mmol/L of L-ascorbic acid-2 phosphates. Assessment of calcium accumulation was visualized by von Kossa staining. For chondrogenesis differentiation, briefly cells were cultured in media supplemented with ITS+1 (Sigma Aldrich), 50 mmol/L L-ascorbic acid-2 phosphates (Sigma Aldrich), 55 mmol/L sodium pyruvate (Invitrogen), 25 mmol/L L-proline (Sigma Aldrich), and 10 ng/mL of transforming growth factor-beta (TGF-b) (Sigma Aldrich). Assessment of proteoglycan accumulation was visualized by alcian blue staining (Sigma Adrich). Adipogenic differentiation was confirmed by the accumulation of neutral lipid vacuoles. Osteogenic differentiation was confirmed in WJSCs by the deposition of a silver-stained mineralized matrix. Chondrogenic differentiation was confirmed by the formation of spheres in the micromass culture and the secretion of cartilage-specific proteoglycans stainable. WJSCs demonstrated a cartilage-like phenotype with chondrocyte-like lacunae (refer
Total RNA was extracted by from WJ-MSCs at SC2 culture using Trizol (Invitrogen) according to the manufacturer's instructions. The RNA was reverse-transcribed into cDNA by using Superscript II reverse transcriptase (Invitrogen) according to the manufacturer's instructions. cDNA amplification was performed in a thermocycler by using Taq polymerase supplied with KCl buffer and 1.5 mmol/L MgCl2 (Invitrogen) at 94° C./1 min, 58° C./30 sec, 72° C./1 min. Polymerase chain reaction (PCR) products were resolved on 1.5% agarose (Invitrogen) gel run in 1× Tris borate-ethylenediaminetetraacetic acid buffer. WJMSCs express pluripotent genes OCT4, REX1, NANOG, STELLA5 and DPPA 5. The culture also express some ectoderm (NESTIN, β-TUB, NF), endoderm (SOX17, GATA2, CK19, CK18, CK8) and mesoderm (GATA4, MSX1, HAND1, BMP4) markers (refer
WJ-MSCs cultures were treated with colcemid 2 hours before harvest, detached by trysinization, and treated with 0.5 mol/L hypotonic solution (KCl/water) before fixing with Conroy's solution (3:1 methanol/glacial acetic acid). The spreads were treated with 0.005% trypsin, stained with Giemsa (Sigma Aldrich), and 20-30 separate metaphase spreads were examined for each culture. WJ-MSCs showed normal karyotypes at passage 2. A representative ideogram is illustrated in
At 80% confluency, WJMSCs were transferred into a non-adherent petri dish containing a neural-inducing medium (NIM) composed of 92% D-MEM/F-12 (1:1), 6000 mg/L D-glucose, 5% KnockOut SR, 2 mM L-glutamine, 1% MEM non-essential amino acids solution, 0.1 mM b-mercaptoethanol, and 1% N2 supplement (all from Gibco BRL). The EBs were well-developed under these conditions.
The cells were cultured on 200 mm cell culture dish (BD Pharmingen, San Diego, Calif.) in Neurobasal A media (GIBCO/Invitrogen, Carlsbad, Calif.) supplemented with B27 (Invitrogen, Carlsbad, Calif.), 20 ng/mL basic fibroblast growth factor (bFGF; Invitrogen) and 20 ng/mL epidermal growth factor (EGF; Invitrogen). Fresh culture medium including EGF and bFGF was added to the medium after 4-5 days of culture.
The cells were induced with a cocktail of 200 ng/mL sonic hedgehog (SHH), 100 ng/mL fibroblast growth factor 8 (FGF8), 10 ng/mL glial cell line-derived neurotrophic factor (GDNF; R&D Systems, Minneapolis, Minn.), and 10 μM forskolin (Sigma). Cells were then cultured at 37° C. with 5% CO 2 for 7 days. Half of the medium was replaced every 2-3 days. After 7 days of cultivation, the cells differentiated into neuronal cells and were tested for neural cell marker expression. WJ-MSCs cell aggregates derived from hanging drop method (
Differentiated cells were fixed with 4% paraformaldehyde for 15 minutes at 25° C. and permeabilised using 0.1% Triton X-100 for 10 minutes at 25° C. Cells were then blocked with blocking buffer (DPBS containing 3% BSA) for 30 minutes at 25° C. and incubated overnight with primary antibodies at 1:500 dilution at 4° C. Primary antibodies used were Nestin-Ms, β-tubulin-Ms, GAD 65&67-Rb and TH-Rb (Abcam®). After three washes with DPBS, cells were incubated with secondary antibodies FITC-conjugated anti-rabbit IgG antibodies (A11012, Molecular probes) and FITC-conjugated anti-mouse IgG antibodies (ab6785, Abcam®). Nucleus was stained with anti-fade 4′,6′-diamidino-2-phenylindole dihydrochloride (DAPI; Chemicon). Observations were made using a fluorescence microscope. Immunochemistry staining for WJMSCs derived neurospheres were positive for nestin and β-tubulin (
| Number | Date | Country | Kind |
|---|---|---|---|
| PI 2015000025 | Jan 2015 | MY | national |
