Viability, yield and expansion capability of feline MSCs obtained from subcutaneous and reproductive organ adipose depots
BMC Veterinary Research volume 17, Article number: 244 (2021)
The source of multipotent stromal cells (MSC) can have a significant influence on the health and expansion capacity of the cells. As the applications for allogeneic MSCs in the treatment of feline diseases increase, the location of the initial donor tissue must be analyzed. To date, comparisons have only been made between feline MSCs collected from bone marrow or abdominal fat. This is the first report to compare cells obtained from different adipose depots in the cat with a focus on clinically relevant donor tissues. The tissue was collected from 34 healthy cats undergoing spaying (fat around the ovaries and uterine horn) or subcutaneous fat collected during surgical procedures.
The amount of starting material is essential to isolate sufficient MSCs. The total tissue yield from the subcutaneous fat was significantly greater than could be obtained from around the reproductive organs, leading to 3 times more MSCs per donor. However, the concentration of MSCs obtained from reproductive fat was higher than from subcutaneous fat. In addition, the viability of the MSCs from the reproductive fat was significantly higher than the subcutaneous fat. Since most spaying occurs in young cats (under 18 months) reproductive fat was collected from adult cats during spaying, illustrating that age did not alter the yield or viability of the MSCs. When sufficient tissue was collected, it was digested either mechanically or enzymatically. Mechanical digestion further decreased the viability and yield of MSCs from subcutaneous fat compared to enzymatic digestion. Biomarkers of stem cell characterization, expansion capacity and function were detected using qPCR. CD70, CD90 and CD105 were all expressed in high levels in the 3 groups. However, the reproductive fat had higher levels of CD73 with the mechanically digested subcutaneous fat having the least. Gata6 was detected in all samples while Sox2 and Sox17 were also detected with higher quantities found in the enzymatically digested subcutaneous fat. Negative control genes of Gata4 and Pdx1 showed no detection prior to 50 cycles. During the first three passages, age of the donor, location of the donor tissue, or digestion protocol had no effect on cell culture doubling times or cell viability.
While MSCs from reproductive fat had superior cells/tissue weight and initial viability, there were still dramatically fewer cells obtained compared to subcutaneous fat due to the limited amount of tissue surrounding the reproductive organs. Further, in P1-P3 cultures there were no differences noted in doubling time or cell viability between tissue obtained from reproductive or subcutaneous fat depots.
Multipotent stromal cells (MSC) are increasingly popular in regenerative medicine because of the ease of access and isolation, ability to self-renew and multipotent potential . These adult stem cells have the ability to differentiate into cells of the mesodermal lineage such as adipocytes and osteoblasts, but they also have transdifferentiation properties allowing them to be driven to other cell types such as neurons or myocardial cells . Reports have described the therapeutic application of MSCs to treat various conditions such as heart failure, inflammatory diseases, musculoskeletal trauma, diabetes and kidney disease . Additionally, MSCs have successfully been used for treating inflammatory conditions such as osteoarthritis or graft versus host disease .
There are numerous clinical applications for MSCs in the veterinary field, including the treatment of feline diseases such as gingivostomatitis, inflammatory bowel disease, allergic asthma and chronic kidney disease [5,6,7,8]. Research on MSC-based treatment for feline ailments is expanding our understanding of the potential of stem cells, along with the challenges associated with feline cells.
MSCs can be harvested from a variety of sources including adipose tissue, bone marrow, peripheral blood, and umbilical cord [9, 10]. Cells from diverse sites have unique properties including basic transcriptome differences and variations in in vitro or in vivo differentiation . Of the multiple sites from which to obtain MSCs, adipose tissue is one of the most commonly used and widely studied. Historically, adipose tissue was considered a simple site of energy storage, but this is no longer the case. Adipose tissue is a functionally dynamic organ that is involved in energy homeostasis and the secretion of several hormones .
The abdominal cavity includes several types of adipose tissue, such as subcutaneous, intramuscular and visceral. Subcutaneous adipose tissue lies underneath the skin and is composed of adipocytes that are organized in lobules, separated by connective tissue. Subcutaneous adipose tissue makes up about 80 % of all body fat . In contrast, visceral adipose tissue is interspersed among the organs and composed of several different depots including mesenteric, perirenal, and fat surrounding the reproductive organs. The MSC characteristics can vary depending on the site of tissue harvest . Reports demonstrate differences in MSC characteristics when comparing subcutaneous and visceral adipose tissue surrounding female reproductive tissue obtained during Caesarean Sections. [15, 16]. Ritter et al. concluded that human visceral fat associated with the reproductive organs had a higher potential to differentiate into adipogenic and osteogenic cells and secreted higher levels of inflammatory cytokines, emphasizing the importance of the site of tissue harvest . Likewise, research in felines has suggested that reproductive fat may have advantages over other fat depots .
While studies have compared feline MSCs obtained from either bone marrow or fat tissue , no study has compared the different abdominal depots of fat for MSC retrieval in cats. When considering the translation of this research to a scaled MSC-based product, we determined that the tissue source should be easily retrieved as part of standard veterinary practice from community-dwelling cats when possible. The objective of the study was to compare feline adipose tissue from subcutaneous and reproductive organ donor sites to test the hypothesis that enzymatically digested reproductive fat would result in higher levels of expansion and multipotent biomarkers along with higher viability and proliferation capabilities.
The study design was a non-randomized subject sample of convenience with tissue collection occurring secondary to standard veterinary clinic procedures. 94 % of the procedures were conducted at licensed veterinary clinics on their clients or at non-profit animal shelters prior to adoption. Only 2 cats were part of research colonies with fat retrieved during procedures related to the other research studies in which they were enrolled.
The average age of the donors in the reproductive group was younger than the subcutaneous group due to the fact that most spaying occurs in pediatric cats. However, 7 spayed cats in the reproductive fat group were over 18 months and thus results of the reproductive fat group were subdivided into pediatric and adult cats to determine whether the age of the donors affected the results. Since all veterinary procedures that allowed the collection of subcutaneous fat occurred on adult cats, there was no pediatric equivalent group. There was no difference in the mean age of the adult cats in the adult reproductive and subcutaneous tissue groups (Table 1). The average body weight was less for the pediatric reproductive group compared to the two adult donor groups (Table 1). Likewise, the body condition scores were statistically greater in the adult subcutaneous tissue donors compared to the other groups (Table 1).
All donors in the reproductive fat group were female, again due to the fact that the fat was obtained during spaying (Table 1). Donors of subcutaneous fat obtained from adult cats were approximately 30 % female, leading to a large difference in the sex distribution between the groups that could not be controlled for.
A far greater quantity of tissue was obtained from the subcutaneous procedure with an average of 9 g of tissue obtained from each animal with a large range of values dependent on the surgical procedure at the time of fat procurement and the preference of the individual veterinarian (Table 1). Approximately 20 times less tissue by weight could be obtained from the adipose tissue surrounding the reproductive organs, regardless of the age of the donor. Interestingly there was no difference in the amount of fat retrieved from the reproductive organs of young or old cats. Tissue harvested from the subcutaneous region of each donor was separated into mechanical or enzymatic digestion. Dual digestion protocols could not be tested using the reproductive fat, due to the limited amount of tissue obtained from each donor. Thus, all reproductive fat samples were enzymatically digested.
While more total tissue was obtained from the subcutaneous region, the yield of live MSCs per gram of tissue was greater for the reproductive fat. Figure 1 illustrates the vast difference in the yield per gram of tissue in the reproductive fat versus the subcutaneous tissue samples, regardless of the age of the reproductive fat donor. To determine whether a different digestion method could rescue the poor live cell yield in the subcutaneous group, we took samples of subcutaneous fat and mechanically digested it. The method of tissue digestion did not alter the results, with mechanical digestion demonstrating the fewest MSCs per tissue weight compared to the two reproductive groups, but no difference than the enzymatically digested subcutaneous samples. Even with the lower density of cells, the vastly larger amount of starting material retrieved from the subcutaneous fat samples still resulted in a larger total number of cells (Table 1).
Harvest Viability and Morphology
Fat cells were plated and 24 h later, the adherent cells were analyzed for viability and morphology. Initial viability following enzymatic digestion of reproductive adipose tissue resulted in over 85 % live cells for both pediatric and adult tissue donors (Fig. 2). In contrast, there was a statistically significant decrease in viability of cells isolated from the subcutaneous tissue. The viability of the cells obtained from subcutaneous fat was approximately 35 % for the mechanical digestion group, while the value was near 55 % for the enzymatic digestion procedure.
Cells from the two harvest sites adhered well to plastic and formed highly homogenous monolayers. All cells took on the expected fibroblast-like spindle appearance (Fig. 3) with the cells from reproductive fat showing the most consistency in shape. There were no noticeable morphological differences between the subcutaneous fat that was enzymatically digested versus mechanical digestion.
Assessment of the extracted RNA demonstrated acceptable quality and concentrations of RNA samples from all groups (Table 2). However, due to limited starting tissue from the reproductive samples, PCR was run on pooled reproductive samples (pediatric and adult). RNA quality met the anticipated 260/280 ratio of > 1.9 for all 3 groups. The 260/230 ratios were less than the anticipated 2.0 but were not statistically different. Verification that the starting material was comprised of MSCs was conducted by examining expression of classic MSC biomarkers using methods previously published [19, 20]. Figure 4 A summarizes the results with high levels of expression of the MSC biomarkers CD73, CD90 and CD105. While CD73 was expressed in the lowest amounts compared to CD90 and CD105, the reproductive fat had the highest expression level of CD73 (lowest ∆Ct value). Subcutaneous enzymatically digested tissue had the highest expression level of CD90. The raw Ct values are provided in supplemental Table 1, confirming the higher expression levels of CD90 and CD105 in all samples. Fragments were run on gels to confirm the correct size (Fig. 4B). The resulting PCR products were purified and sent to Genewiz for sequencing. All results matched the expected sequences and sizes (Table 3).
In order to assess differences in the multipotency of the cells, we examined the early differentiation markers GATA4 involved in embryogenesis of the mesoderm and endoderm , GATA6 a mesodermal marker involved in regulation of cell differentiation , SOX2 essential for pluripotency maintenance in stem cells  and SOX17 involved in the regulation of embryonic development .
Gata4 expression was low in all 3 samples (Fig. 5 A). with the cells from reproductive fat showing more expression than the other 2 groups (lower ΔCt). As expected, Gata6 expression was high in the feline cells. The digestion method did affect Gata6 expression as the enzymatic and the mechanical digestion performed similarly. Sox2 expression was greatest in the cells digested enzymatically, showing lesser amplification in the mechanically digested samples (Fig. 5 A). Expression of Sox17 followed the same trend as Sox2 expression, demonstrating an increase in expression in the enzymatically digested tissue. PDX1 is a marker of early human pancreatic development as is typically only detected in late endoderm differentiation . After failing to detect significant levels of Gata4 in the feline adipose tissue, we added the analysis of Pdx1 as a negative control. As expected, Pdx1 was detected only after extremely high cycle numbers, and normalization to Gapdh did not change the results (Fig. 5 A).
Because both Gata4 and Pdx1 were consistently detected but at high cycle levels (> 35 cycles), the fragment sizes were evaluated to ensure that they were the correct size and not primer dimers or contaminants. Figure 5B provides examples of the amplicons showing the anticipated size for all of the biomarkers with no additional bands present. The gels were cropped to provide a standard order for the groups. The full gels are provided in the supplemental section of this manuscript (Figure S1). In addition, the amplicons were sequenced showing a match with the expected results (Table 3). In order to appreciate the level of expression, the raw Ct values are provided in Supplemental Table 2.
Cell Culture Expansion
To measure any effects of the different donor characteristics on cell culture expansion, cells were seeded at an approximate density of 5,000 cells/cm2 and cell expansion measured by population doubling times. Figure 6 A summarizes the differences in expansion capability for the four groups. During P1-P3, there were no significant differences between the groups’ mean doubling time. Interestingly, all groups showed a trend towards longer doubling times with subsequent passages, except for the cells obtained from adult cat subcutaneous tissue and mechanically digested, which had a slight decrease in doubling time with each passage.
Viability of the cells was measured at the end of each passage. The cells in these groups showed high viability with no differences between groups (Fig. 6B).
MSCs are becoming increasingly relevant to clinical care  but the outcomes associated with MSC treatment have shown great inconsistency. Some of the outcome variability may be due to the altered characteristics associated with the donors such as age and sex and based on the site of isolation of the initial tissue . Other factors responsible for inducing variability may include the methods of isolation, the amount of tissue harvested, and the passage number. In felines, there have been few studies to compare sources of MSCs and they have focused on comparing bone marrow-derived MSC to adipose MSCs . Further, when working with abdominal adipose tissue, the exact donor site often is not clarified in the reports [27, 28]. A unique study design was undertaken to enhance the translation of the data to the clinical setting. The tissue was retrieved during veterinary standard procedures, either abdominal surgery or spaying of female cats and, when possible, the settings were either licensed clinical veterinary practices or animal shelters.
Obviously, a much greater quantity of adipose tissue can be harvested from the subcutaneous fat depot as compared to the reproductive depot. However, the density of MSCs obtained from those regions was vastly different with the tissue surrounding the reproductive organs resulting in 40 times more MSCs per tissue weight. Differences in the age of the female cats had no effect on the yield of cells from reproductive fat. Even with this great difference in yield (cells per tissue weight), the overall number of cells obtained was greater with the subcutaneous harvest due to the large volume of subcutaneous fat that could be retrieved. However, subcutaneous cells had an extremely low viability, especially when digested mechanically, along with the slowest P2 doubling time. The range of doubling times reported here are consistent with some previous publications of feline abdominal adipose tissue  but slower than those reported by others [30, 31].
Only one other group has focused on different fat depots in felines comparing abdominal from subcutaneous locations . They found that there was no difference between the two locations in the multipotent markers nor in the ability of the cells to differentiate into mesoderm lineages. However, they did not identify the exact location of the abdominal fat depot, thus it is difficult to directly compare their results to those reported here.
There have been reports suggesting that mechanical digestion can be advantageous to enzymatic digestion when small quantities of MSCs are desired due to its decreased cost and time commitment but with a decreased yield . We confirmed that the yield for the mechanically digested sample was significantly less than the other 2 groups and the resulting viability of the cells was poor (approximately 25 %). While the remaining cells could be rescued and passaged, the poor initial outcome indicates that a significantly larger amount of starting material would be necessary to harvest, if using mechanical digestion.
The quality and amount of RNA extracted from the groups showed no relevant differences. This is important because previous studies concluded that fat contains a high fatty acid content that can interfere with the extraction of pure RNA, indicated by the 260/230 ratio . We were able to confirm the identity of the starting cells as MSC based on their biomarker signature described by previous publications [18, 19, 27, 29, 31]. While all three groups presented with high levels of expression of standard MSC biomarkers, the reproductive fat sample had the highest level of CD73 while the subcutaneous enzymatic sample had more CD90, although these differences were likely not clinically relevant. We further investigated the pluripotency and lineage assignment potential to further characterize the tissue using previously published techniques [19, 27]. While the differences in expression levels of some of the pluripotent biomarkers reached statistical significance, the differences were small and likely not biologically relevant. Importantly, all of the pluripotency biomarkers were detected at high CT values, indicating low levels of gene expression.
SOX2 is a master stem cell transcription factor, determining the stemness capacity of cells . While high levels of expression of SOX2 have been reported in human, monkey and canine abdominal fat previously [34, 35], its detection in feline cells has been variable. Cat embryos, along with undifferentiated feline neural stem cells, contain high levels of Sox2 [36,37,38]. In addition, a number of labs have shown that induced pluripotent stem cells derived from feline fibroblasts express Sox2 [39, 40]. In comparison with canine cells, feline amniotic MSCs showed a much lower expression of Sox2 and less immunostaining of the protein compared to canine amniotic stem cells . Some have reported the inability to detect Sox2 or the resulting protein in feline abdominal or subcutaneous adipose MSCs [27, 28]. In contrast, our results are consistent with those of Lee et al., showing detection of Sox2 in the abdominal adipose tissue . Unfortunately, ours is the only study to include the raw Ct values of our results rather than relative values that provide no indication of the absolute levels.
GATA6 encodes a transcription factor normally found in MSCs essential to the self-renewal properties of pluripotent cells. Knockdown of GATA6 results in suppression of the self-renewal capacity of MSCs . In cats, Gata6 is assumed to be involved in differentiation similar to humans, but that has yet to be examined. Studies have described the presence of Gata6 in feline induced pluripotent stem cells  and in cat embryos , but ours is the first study to report the presence of Gata6 in feline adipose MSCs.
SOX17, identified in human adipose derived MSCs , is involved in the capacity of the cells to differentiate into endoderm and eventually to hepatocytes  or pancreatic tissue . Like Gata6, Sox17 has been detected in feline induced pluripotent stem cells , but has not been investigated in feline adipose MSCs. Thus, this is the first study to identify Sox17 in feline adipose-derived MSCs.
GATA4 is found in high levels in human ovaries where it is associated with sex determination along with ovary growth and function, but not in adipocytes . GATA4 is involved in differentiation into osteoblasts and development of the heart and has been reported to be expressed in only 15 % of rat bone marrow-derived MSCs based on immunohistochemistry . Thus, it was not surprising that little was detected in the adipose MSCs. In fact, minimal expression confirmed that ovarian tissue did not contaminate the reproductive fat group. Likewise, PDX1 is a biomarker of pancreatic development and is farther down the differentiation lineage. We included Pdx1 detection as a negative control, thus the lack of Pdx1 was expected.
A major limitation of the study was the fact that because the reproductive fat was obtained during spaying, there was a difference in the sex distribution between groups. Based on a clinically relevant study design that collected excess tissue from standard procedures on predominantly community dwelling cats, sex could not be controlled for as a variable. A much larger clinical study is warranted to determine possible sex-based differences. In addition, this study did not analyze the purity or differentiation capacity of the cells at any of the passages.
While cells from all three groups studied here had similar pluripotency profiles, the improved yield (cells/tissue weight) and initial cell viability was dramatically better for the cells harvested from the reproductive tissue, which can be harvested ethically during spaying procedures. If the goal is an autologous product, then reproductive fat harvests would not be appropriate, but the field is quickly moving toward the allogeneic model. Consequently, fat surrounding the reproductive organs may offer a consistently high-quality source of MSCs. In addition, we showed that enzymatic digestion was the best approach for subcutaneous tissue and the only option available when working with reproductive tissue due to the small amount of starting material.
In conclusion, the work summarized here demonstrates that feline reproductive adipose tissue is a reasonable source of MSCs to be cultured for eventual therapeutic application compared to a subcutaneous fat depot. The age of the donor did not affect the quality of the MSCs from the reproductive fat. The MSCs should be isolated via predominantly enzymatic digestion, but further research should be done to continue optimizing a digestion protocol. For example, in certain clinical situations, long-term cell culture may not be possible and mechanically-digested subcutaneous fat may be the only option. In addition, further research should continue to further characterize feline adipose-derived MSC, including the differentiation potentials.
Adipose Tissue Collection
The adipose tissue was collected from 34 healthy female cats, including cats undergoing spaying at local animal shelters and the discarded tissue removed during spaying (the ovaries and uterine horn) was collected and the fat dissected. Subcutaneous fat was removed from male and female cats under anesthesia for unrelated surgical procedures. Additionally, two samples were obtained from research animals undergoing euthanasia (sodium pentobarbital) at the completion of an unrelated study. The University of Kansas Medical Center’s IACUC determined that tissue removed during spaying or after euthanasia was exempt from required protocol approval. As all tissue collected would otherwise have been discarded, no consent was necessary. The licensed veterinarians overseeing the animals approved the collection of the discarded tissue. No exclusion criteria were set for the study. Table 1 summarizes the donor characteristics. All donors were standard long or shorthair cats and were fully immunized at the time of tissue retrieval. Due to the fact that tissue was retrieved during other procedures, the site of tissue collection (reproductive versus subcutaneous) could not be randomized. Group assignments were based on convenience of the surgical procedures completed through the duration of the study. Due to large differences in the tissue mass obtained from the different sites, blinding of the initial sample groups could not be done. Analysis of the later passages was completed in a blinded fashion. Donor characteristics were provided by the attending veterinarian and included age, weight, sex, body condition, vaccination history, and general health status including feline leukemia virus results.
For subcutaneous fat collection, donors were positioned in dorsal recumbency and the surgical site was prepared using standard aseptic surgical procedures. A 1 cm length incision was made at the midline to allow access to fat deposits in the ventral abdomen. Using a Tulip multi-port tissue harvester cannula attached to a 60CC syringe the abdominal fat was broken up with gentle back and forth movement of the cannula device. The syringe was then used to draw out the fat tissue that was transferred to collection media, consisting of Dulbecco’s Modified Eagle’s Medium (DMEM) supplemented with 1 % pen strep.
Reproductive adipose tissue was collected aseptically during standard spaying of healthy cats. The removed ovaries and uterine horn were placed in chilled transport medium comprised of DMEM/F12 (ThermoFisher, Cat#124,000,024) containing 1 % Penicillin-Streptomycin (ThermoFisher, Cat#15,140,122) and transported to the lab on ice. Under aseptic conditions, the fat was manually dissected from the reproductive organs.
Digestion of Adipose Tissue
Under aseptic conditions, the tissue was rinsed, weighed, and minced using sterile scissors. Mechanical digestion involved passing the adipose tissue between two 60 mL syringes connected with an anaerobic luer-to-luer connector (Tulip, Cat #TP ATLLLL2.4). Using the 2.4 mm Tulip connector, the tissue was passed between the two syringes 10 times and then passed through the smaller 1.2 mm Tulip connector (Tulip, Cat#TP ATLLLL1.2) another 10 times. The tissue solution was centrifuged at 550xg for 10 min. The cell pellet was reserved for plating in DMEM culture medium. The remaining supernatant was collected and the digestion was repeated twice more with increasing centrifugation speeds in each round of digestion (620xg and 690xg, respectively). The cells from the pellets from each digestion were collected and counted. The pellets were resuspended in DMEM:F12 with 10 % FBS (ThermoFisher, Cat #26,140,087) and 1 % Penicillin-Streptomycin and cultured at 37 °C, 5 % CO2 in a humidified chamber.
Under aseptic conditions, the tissue was rinsed, weighed, and minced using sterile scissors and digested in a 0.6 WU/mL Liberase (Roch, Liberase MNP-S, /cat #06297790001) for 30 min at 37 °C. For the larger tissue amounts of subcutaneous fat, the tissue was passed through a 100 mm filter and centrifuges at 260xg for 5 min. The supernatant was removed and mixed with 5 mL of red blood cell lysis buffer (Millipore Sigma, Cat #11,814,389,001) followed by centrifugation at 260xg for 5 min. The final supernatant was resuspended in DMEM:F12 with 10 % FBS and 1 % Penicillin-Streptomycin and cultured at 37 °C, 5 % CO2 in a humidified chamber.
Following digestion, cells were incubated for 48 h at 37 °C and 5 % CO2 after which the non-adherent cells were removed, and fresh medium was added. The remaining plastic-adherent cells were trypsinized (Worthington Cat# 9002-07-7) and re-plated at a density of 5,000 cells/cm2 into T175 flasks. Cell numbers were calculated using automated cell counter (EVE; NanoEnTek) at the time of passage and during expansion in order to calculate the doubling time. Cells were passaged when they met the requirement of 80–100 % confluency. Flasks that failed to obtain 80 % confluency were removed from analysis. Images of cultured cells were obtained using an Axio Vert.A1 Inverted microscope (Zeiss) with a 10X objective. Cells were not cultured beyond 5 passages.
Doubling time was calculated based on a published protocol .
T is time, ln is the natural log, Xb indicates the starting cell number, and Xe indicates the ending cell number.
Viability was measured from fluorescence emission levels of calcein (ThermoFisher, Cat #C3099) and propidium iodide (ThermoFisher, Cat #P3566) on a multi-mode plate reader (BioTek Cytation 5). Calcein stains live cell green and PI stains dead cells as red. Viability was calculated as:
Trypan blue exclusion staining was also used as a measure of viability. The cells were dispersed into single cell suspensions using trypsin and briefly incubated with Trypan blue. Viability was determined as the ratio of (live cells / total number of cells) x 100.
Total RNA was extracted from frozen cell pellets of the digested adipose tissue using the mirVana RNA Extraction kit (ThermoFisher, Cat#AM1560) per the manufacturer’s protocol. RNA quality was assessed using the NanoDrop 1000 Spectrophotometer (Thermo-Fisher). Absorbance was read at 230, 260 and 280 nm. The 260/280 ratio of ~ 2.0 indicates high quality RNA. Likewise, a 260/230 ratio of between 2.0 and 2.2 indicates a pure sample.
One µg of total RNA was used to make cDNA using SuperScript IV Reverse Transcriptase (Invitrogen, Cat #18,090,010) as per the manufacturer’s protocol using oligo (dT). Primer sequences for the biomarkers were determined using BLAST (Table 3) and confirmed via gel electrophoresis.
The cDNA was run through RT-qPCR on the Applied Biosystems ViiA7 PCR System using Power SYBR Green PCR Master Mix (Applied Biosystems, Cat #4,367,659) using the following protocol: 2 min at 95℃ for initial denaturation, followed by cycling 15 s at 95℃ for denaturation, 10 s at 60℃ for annealing, and 60 s at 70℃ for extension. This protocol repeated for 49 cycles, followed by recording a melt curve. All samples were amplified in triplicate. An automatic threshold was utilized and a cut off of 40 cycles was determined to indicate presence or absence of biomarkers. Negative controls without template were run to 50 cycles with no amplification. The cycle threshold values were normalized to Gapdh. To confirm the results, amplicons were run on gels to confirm the correct sizes. In addition, the resulting PCR products were purified and sent to Genewiz for Sanger sequencing. All results matched the expected sequences and sizes (Table 3).
Data were analyzed using a one-way analysis of variance (ANOVA) on ranks with post hoc Dunn’s pairwise comparison was performed using SigmaPlot 13.0. P values of less than 0.05 were considered statistically significant, noted by symbols in the graphs. Data are presented as averages ± SEM.
Availability of data and materials
Data generated and analyzed for the current study are available from the corresponding author.
- CO2 :
- cm2 :
Cluster of differentiation
Change in Ct
Dulbecco’s Modified Eagle Medium F-12
multipotent stromal cells
- P1, P2 or P3:
Quantitative reverse transcription polymerase chain reaction
Starting cell number
Ending cell number
Zomer H, Vidane A, Goncalves N, Ambrosio C. Mesenchymal and induced pluripotent stem cells: general insights and clinical perspectives. Stem Cells Cloning. 2015;8:125–34.
Golpanian S, Wolf A, Hatzistergos K, Hare J. Rebuilding the Damaged Heart: Mesenchymal Stem Cells, Cell-Based Therapy, and Engineered Heart Tissue. Physiol Rev. 2016;96:1127–68.
Peng Y, Ke M, Xu L, Liu L, Chen X, Xia W, et al. Donor-derived mesenchymal stem cells combined with low-dose tacrolimus prevent acute rejection after renal transplantation: a clinical pilot study. Transplantation. 2013;85(1):161–8.
Regmi S, Pathak S, Kim J, Yong C, Jeong J. Mesenchymal stem cell therapy for the treatment of inflammatory diseases: Challenges, opportunities, and future perspectives. Eur J Cell Biol. 2019;98:151041.
Marx C, Silveira M, Nardi N. Adipose-derived stem cells in veterinary medicine: characterization and therapeutic applications. Stem Cells Devel. 2015;24(7):803–13.
Trzil J, Masseau I, Webb T, Chang C-H, Dodam J, Liu H, et al. Intravenous adipose-derived mesenchymal stem cell therapy for the treatment of feline asthma: a pilot study. J Feline Med Surg. 2016;18(12):981–90.
Quimby J, Borjesson D. Mesenchymal stem cell therapy in cats: current knowledge and future potential. J Feline Med Surg. 2018;20:208–16.
Thomson A, Berent A, Weisee C, Langston C. Intra-arterial renal infusion of autologous mesenchymal stem cells for treatment of chronic kidney disease in cats: phase I clinical trial. J Vet Int Med. 2019;33(3):1351–61.
Sato K, Yamawaki-Ogata A, Kanemoto I, Usui A, Narita Y. Isolation and characterization of peripheral blood-derived feline mesenchymal stem cells. Vet J. 2016;216:183–8.
Zazzeroni L, Lanzoni G, Pasquinelli G, Ricordi C. Considerations on the harvesting site and donor derivation for mesenchymal stem cells-based strategies for diabetes. CellR4 Repair Replace. Regen Reprogram. 2017;5(5):e2435.
Lavrentieva A, Hoffmann A, Lee-Thedieck C. Limited potential or unfavorable manipulations? Strategies toward efficient mesenchymal stem/stromal cell applications. Front Cell Dev Biol. 2020;8:316.
Coelho M, Oliveira T, Fernandes R. Biochemistry of adipose tissue: an endocrine organ. Arch of Med Sci. 2013;9:191–200.
Ibrahim M. Subcutaneous and visceral adipose tissue: structural and functional differences. Obes Rev. 2010;11:11–8.
Guercio A, Di Bella S, Casella S, Di Marco P, Russo C, Piccione G. Canine mesenchymal stem cells (MSCs): characterization in relation to donor age and adipose-tissue-harvesting site. Cell Biol Int. 2013;37(8):789–98.
Ritter A, Friemel A, Roth S, Kreis N, Hoock S, Safdar B, et al. Subcutaneous and Visceral Adipose-Derived Mesenchymal Stem Cells: Commonality and Diversity. Cells. 2019;8(10):1288.
Voga M, Adamic N, Vengust M, Majdic G. Stem Cells in Veterinary Medicine - Current State and Treatment Options. Front Vet Sci. 2020;7:278.
Fargason C, Zhang N, Lopez M. Feline adult adipose tissue-derived multipotent stromal cell isolation and differentiation. In: Brunnell B, Gimble J, editors. Adipose-Derived Stem Cells: Methods and Protocols, Methods in Molecular Biology. 1773. New York: Humana Press; 2018. pp. 173–88.
Webb T, Quimby J, Dow S. In vitro comparison of feline bone marrow-derived and adipose tissue-derived mesenchymal stem cells. J Feline Med Surg. 2012;14:165–8.
Cardoso M, Pinheiro A, Vidane A, Casals J, de Oliveira V, Goncalves N, et al. Characterization of teratogenic potential and gene expresssion in canine and feline amniotic membrane-derived stem cells. Reprod Dom Aniim. 2017;52:58–64.
Rutigliano L, Corradetti B, Valentini L, Bizzaro D, Meucci A, Cremonesi F, et al. Molecular characterization and in vitro differentiation of feline progenitor-like amniotic epithelial cells. Stem Cell Res Ther. 2013;4(5):133.
Mangi A, Noiseux N, Kong D, He H, Rezvani M, Ingwall J, et al. Mesenchymal stem cells modified with Akt prevent remodeling and restore performance of infarcted hearts. Nat Med. 2003;9(9):1195–201.
Sagi B, Marahgechi P, Urban V, Hegyi B, Szigeti A, Fajka-Boja R, et al. Positional identity of murine mesenchymal stem cells resident in different organs is determined in the postsegmentation mesoderm. Stem Cells Devel. 2012;21(5):814–28.
Kozlowska U, Krawczenko A, Futoma K, Jurek T, Rorat M, Patrzalek D, et al. Similarities and differences between mesenchymal stem/progenitor cells derived from various human tissues. World J Stem Cells. 2019;11(6):347–74.
Kanai-Azuma M, Kanai Y, Gad J, Tajima Y, Taya C, Kurohmaru M, et al. Depletion of definitive gut endoderm in Sox17-null mutant mice. Development. 2002;129(10):2367–79.
Zhu Y, Liu Q, Zhou Z, Ikeda Y. PDX1, Neurogenin-3, MAFA: critical transcription regulators for beta cell development and regeneration. Stem Cell Res Ther. 2017;8:240.
Wada Y, Ikemoto T, Morine Y, Imura S, Saito Y. S Y, et al. The Differences in the Characteristics of Insulin-producing Cells Using Human Adipose-tissue Derived Mesenchymal Stem Cells from Subcutaneous and Visceral Tissues. Sci Rep. 2019;9:13204.
Gomez M, Qin Q, Biancardi M, Galiguis J, Dumas C, MacLean R, et al. Characterization and multilineage differentiation of domestic and black-footed cat mesenchymal stromal/stem cells from abdominal and subcutaneous adipose tissue. Cell Reprogam. 2015;17(5):376–92.
Kim H-R, Lee J, Byeon J, Gu N-Y, Lee J, Cho I-S, et al. Extensive characterization of feline intra-abdominal adipose-derived mesenchymal stem cells. J Vet Sci. 2017;18(3):299–306.
Clark K, Fierro F, Ko E, Walker N, Arzi B, Tepper C, et al. Human and feline adipose-derived mesenchymal stem cells have comparable phenotype, immunomodulatory functions, and transcriptome. Stem Cell Res Ther. 2017;8:69.
Panasophonkul S, Samart P, Kongon K, Sathanawongs A. Phenotypic characteristics of feline adipose-derived stem cells affected by cell passage numbe. Pol J Vet Sci. 2017;20(4):651–60.
Lee B-Y, Li Q, Song W-J, Chae H-K, Kweon K, Ahn J-O, et al. Altered properties of feline adipose-derived mesenchymal stem cells during continuous in vitro cultivation. J Vet Med Sci. 2018;80(6):930–8.
Aronowitz J, Lockhart R, Hakakian C. Mechanical versus enzymatic isolation of stromal vascular fraction cells from adipose tissue. Springerplus. 2015;4:713.
Spence J, Lange A, Lin S, Kaestner K, Lowy A, Kim I, et al. Sox17 regulates organ lineage segregation of ventral foregut progenitor cells. Dev Cell. 2009;17(1):62–74.
Izadpanah R, Trygg C, Patel B, Kriedt C, Dufour J, Gimble J, et al. Biologic properties of mesenchymal stem cells derived from bone marrow and adipose tissue. J Cell Biochem. 2006;99:1286–97.
Takemitsu H, Zhao D, Yamamoto I, Harada Y, Michishita M, Arai T. Comparison of bone marrow and adipose tissue-derived canine mesenchymal stem cells. BMC Vet Res. 2012;8:150.
Filliers M, Goossens K, VanSoom A, Merlo B, Pope C, De Rooster H, et al. Gene expression profiling of pluripotency and differentiation -related markers in cat oocytes and preimplantation embryos. Reprod Fertil Dev. 2012;24(5):691–703.
Alexanian A, Crowe M, Kurpad S. Efficient differentiation and integration of lineage-restricted neural precursors in the traumatically injured adult cat spinal cord. J Neuroscie Meth. 2006;150:41–6.
Klassen H, Schwartz P, Ziaeian B, Nethercott H, Young M, Bragadottir R, et al. Neural precursors isolated from the developoing cat brain show retinal integration following transplantation to the retina of the dystrophic cat. Vet Ophthalmol. 2007;10(4):245–53.
Dutton L, Dudhia J, Guest D. Inducing pluripotency in the domestic cat (felis catus). Stem Cells Devel. 2019;28(19):1299–309.
Zhou T, Guo S, Zhang Y, Wang Y, Wang L, Ma J. GATA4 regulates osteoblastic differentiation and bone remodeling via p38-mediated signaling. J Mol Histol. 2017;48:187–97.
Kubo H, Shimizu M, Taya Y, Kawamoto T, Michia M, Kaneko E, et al. Identification of mesenchymal stem cell (MSC)-transcription factors by microarray and knockdown analyses and signature molecule-marked MSC in bone marrow by immunohistochemistry. Genes Cells. 2009;14(3):407–24.
Zhou T, Comizzoli P, Keefer C. Endogenous pluripotent factor expression after reprogramming cat fetal fibroblasts using inducible transcription factors. Mol Reprod Dev. 2019;86(11):1671–81.
Poloni A, Maurizi G, Leoni P, Serrani F, Mancini S, Frontini A, et al. Human dedifferentiated adipocytes show similar properties to bone marrow-derived mesenchymal stem cells. Tissue-Specific Stem Cells. 2012;30(5):965–74.
Buyl K, Vanhaecke T, Desmae T, Lagneaux L, Rogiers V, Najar M, et al. Evaluation of a new standardized enzymatic isolation protocol for human umilical cord-derived stem cells. Toxicol in Vitro. 2015;29(6):1254–62.
Tremblay M, Sanchez-Ferras O, Bouchard M. GATA transcription factors in development and disease. Development. 2018;145:dev164384.
Korzynska A, Zychowica M. A method of estimation of the cell doubling time on basis of the cell culture monitoring data. Biocybernetics Biomed Eng. 2008;28(4):75–82.
The authors wish to acknowledge S. Janette Williams and Dr. Nataliya Kibiryeva for support throughout the project.
Financial support for the fellowship of Dr. P. Ortiz was provided by the Young Leaders of the Americas Initiative. Research funding was supplied by the Kansas City University Student Research Fund. The funding bodies played no role in the design, analysis or reporting of the study.
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Wysong, A., Ortiz, P., Bittel, D. et al. Viability, yield and expansion capability of feline MSCs obtained from subcutaneous and reproductive organ adipose depots. BMC Vet Res 17, 244 (2021). https://doi.org/10.1186/s12917-021-02948-0