Skip to main content
Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Characterization and Immunomodulatory Effects of Canine Adipose Tissue- and Bone Marrow-Derived Mesenchymal Stromal Cells

  • Keith A. Russell ,

    Affiliation Departments of Biomedical Sciences, Ontario Veterinary College, University of Guelph, Guelph, Canada

  • Natalie H. C. Chow,

    Affiliation Departments of Biomedical Sciences, Ontario Veterinary College, University of Guelph, Guelph, Canada

  • David Dukoff,

    Affiliation Departments of Biomedical Sciences, Ontario Veterinary College, University of Guelph, Guelph, Canada

  • Thomas W. G. Gibson,

    Affiliation Clinical Studies, Ontario Veterinary College, University of Guelph, Guelph, Canada

  • Jonathan LaMarre,

    Affiliation Departments of Biomedical Sciences, Ontario Veterinary College, University of Guelph, Guelph, Canada

  • Dean H. Betts,

    Affiliation Physiology and Pharmacology, The University of Western Ontario, London, Canada

  • Thomas G. Koch

    Affiliations Departments of Biomedical Sciences, Ontario Veterinary College, University of Guelph, Guelph, Canada, The Orthopaedic Research Lab, Aarhus University, Aarhus, Denmark



Mesenchymal stromal cells (MSC) hold promise for both cell replacement and immune modulation strategies owing to their progenitor and non-progenitor functions, respectively. Characterization of MSC from different sources is an important and necessary step before clinical use of these cells is widely adopted. Little is known about the biology and function of canine MSC compared to their mouse or human counterparts. This knowledge-gap impedes development of canine evidence-based MSC technologies.

Hypothesis and Objectives

We hypothesized that canine adipose tissue (AT) and bone marrow (BM) MSC (derived from the same dogs) will have similar differentiation and immune modulatory profiles. Our objectives were to evaluate progenitor and non-progenitor functions as well as other characteristics of AT- and BM-MSC including 1) proliferation rate, 2) cell surface marker expression, 3) DNA methylation levels, 4) potential for trilineage differentiation towards osteogenic, adipogenic, and chondrogenic cell fates, and 5) immunomodulatory potency in vitro.


1) AT-MSC proliferated at more than double the rate of BM-MSC (population doubling times in days) for passage (P) 2, AT: 1.69, BM: 3.81; P3, AT: 1.80, BM: 4.06; P4, AT: 2.37, BM: 5.34; P5, AT: 3.20, BM: 7.21). 2) Canine MSC, regardless of source, strongly expressed cell surface markers MHC I, CD29, CD44, and CD90, and were negative for MHC II and CD45. They also showed moderate expression of CD8 and CD73 and mild expression of CD14. Minor differences were found in expression of CD4 and CD34. 3) Global DNA methylation levels were significantly lower in BM-MSC compared to AT-MSC. 4) Little difference was found between AT- and BM-MSC in their potential for adipogenesis and osteogenesis. Chondrogenesis was poor to absent for both sources in spite of adding varying levels of bone-morphogenic protein to our standard transforming growth factor (TGF-β3)-based induction medium. 5) Immunomodulatory capacity was equal regardless of cell source when tested in mitogen-stimulated lymphocyte reactions. Priming of MSC with pro-inflammatory factors interferon-gamma and/or tumour necrosis factor did not increase the lymphocyte suppressive properties of the MSC compared to untreated MSC.


No significant differences were found between AT- and BM-MSC with regard to their immunophenotype, progenitor, and non-progenitor functions. Both MSC populations showed strong adipogenic and osteogenic potential and poor chondrogenic potential. Both significantly suppressed stimulated peripheral blood mononuclear cells. The most significant differences found were the higher isolation success and proliferation rate of AT-MSC, which could be realized as notable benefits of their use over BM-MSC.


Mesenchymal stromal cells (MSC) have progenitor and non-progenitor categories of function that show promise for their clinical use in a wide variety of conditions. Progenitor function refers to the cells' multipotency or their ability to be directed into several cell types including those that make up fat, bone, and cartilage. Non-progenitor function refers to the cells' more recently discovered ability to influence resident cells and tissue functions through their secretome and direct cell-cell contact, including regenerative and immune modulatory effects [1]. These two types of function along with MSC' readiness for in vitro expansion have led to much interest from scientists and clinicians alike. Recently, the dog has emerged as an increasingly useful preclinical animal model to study the development and safety of stem cell–based therapies. Comprehensive validation of the utility of canine MSC will provide far-reaching benefit in both the veterinarian field as well as in translational medicine.

The heterogeneity of MSC populations makes definitive characterization inherently challenging. The International Society for Cellular Therapy attempted to simplify this by establishing three criteria to define the MSC: 1) plastic-adherence, 2) specific positive and negative expression of a panel of specific cell surface markers, and 3) trilineage differentiation potential into bone, cartilage, and fat [2]. Unfortunately, while the first criterion is universal enough for cross-species application, the second criterion's surface marker panel is based on human MSC. A corresponding panel for canine MSC is yet to be established, but progress is being made with markers such as CD44 and CD90 showing consistent positive and CD34 and CD45 consistent negative expression [3].

Adipogenesis and osteogenesis are frequently shown in canine MSC studies most often validated with histological staining and sometimes with mRNA expression data of induced versus non-induced MSC populations [3]. Chondrogenic induction of canine MSC has proven challenging using standard protocols and robust chondrogenic differentiation remains to be shown [417]. Even in our own previous attempts, we were unable to successfully induce chondrogenesis in our canine cells [18]. However, all of this may be less damaging to the clinical utility of MSC as a paradigm shift directs focus to their non-progenitor functions [19,20].

Early in this century, reports began to emerge of the ability of MSC derived from bone marrow aspirate (BM-MSC) to suppress proliferation of T-lymphocytes after stimulation with allogeneic cells or mitogens [21,22]. Soon after, adipose tissue-derived (AT-)MSC were shown to have similar immunomodulatory properties as their bone marrow-derived counterparts [23]. It has been suggested that MSC effect this immunosuppression through cell-cell contact and secreted soluble factors [2427]. While some factors are constitutively expressed, others like indoleamine 2,3-dioxygenase (IDO) are induced by pro-inflammatory cytokines such as interferon-gamma (IFN-γ) and tumour necrosis factor-alpha (TNF-α) [28,29]. While activated T-lymphocytes produce IFN-γ and TNF-α, pre-licensing or priming MSC with these inducers in culture promote their immunosuppressive properties [2832]. Only a few articles on canine MSC immune modulation have been published [3336], and no comparison of canine AT- and BM-MSC with regards to their immunomodulatory function has been reported, nor have the effects of proinflammatory cytokine-primed canine MSC been studied to date.

In this study, we examined both the progenitor and non-progenitor functions of canine AT- and BM-MSC. Surface marker expression, population doubling times, and DNA methylation quantification were also compared for the purpose of explaining any differences between the cell sources with regards to their differentiation or immunomodulatory capacities.


Donor paired canine adipose tissue (AT)- and bone marrow (BM)-derived MSC will have similar differentiation capacity and immune modulatory properties.


To characterize AT- and BM-derived MSC with regards to their:

  1. Population doubling time
  2. Cell surface marker expression
  3. Global DNA methylation quantification
  4. Trilineage differentiation potential
  5. Immunomodulatory potency

Materials and Methods

Ethics statement

Guidelines by the University of Guelph Animal Care Committee were closely followed with regard to the collection of canine blood, adipose tissue, and bone marrow samples. Since collection of these tissue samples occurred post-mortem and dogs were sacrificed for reasons unrelated to the studies, subsequent research conducted using these samples did not require review by the Animal Care Committee (falls under CCAC Category of Invasiveness A). Therefore, these studies were conducted in accordance with the institutional ethics guidelines. Blood and tissues were collected immediately after the dogs were euthanized by intravenous injection of pentobarbital (Euthanyl Forte, 540mg/5 Kg, Biomeda-MTC Animal Health, Cambridge, Ontario) at Hillside Kennels Animal Control, Innerkip, ON. Euthanasia was deemed necessary by the kennel as the dogs were aggressive/dangerous and not suitable for adoption.

MSC isolation

Cryopreserved AT- and BM-MSC were thawed from previously isolated and cryopreserved cultures from 8 dogs [18]. The dogs used were of unknown age each weighing a minimum 30 kg.

MSC culture and proliferation

MSC were cultured in expansion medium (EM) composed of low glucose Dulbecco’s modified Eagle’s medium (DMEM, Lonza, Walkersville, Maryland), 10% pooled FBS (Life Technologies, Grand Island, New York), 1% penicillin/streptomycin, and 1% L-glutamine (Lonza, Walkersville, Maryland) and incubated at 38°C in a 5% CO₂ humidified environment. Cells were harvested at 60–80% confluency using a cell detachment solution (Accumax, Innovative Cell Technologies, San Diego, California) and counted with an automated cell counter (Nucleocounter NC100, Mandel Scientific, Guelph, Ontario). Population doubling times were calculated from passage 2 through passage 5 (AT-MSC, n = 8; BM-MSC, n = 6). For all the following experiments, MSC from passages 3–6 were used for this study.


Canine MSC (n≥3 for each cell source) were analyzed for surface marker expression using the Accuri C6 flow cytometer and software (BD, Mississauga, ON). Canine peripheral blood mononuclear cells (PBMC, n≥1) were used as controls. The antibodies used are listed in Table 1. All antibodies utilized were canine-specific except for MHC I (bovine) and CD73 (human), which were stated to cross-react with canine cells by the manufacturers and were validated with bovine and human PBMC respectively. Unstained samples of each MSC and PBMC were gated to determine surface marker expression of their stained counterparts.

Global DNA methylation quantification

Genomic DNA was isolated from AT- and BM-MSC samples (AT-MSC, n = 6; BM-MSC, n = 6) using a column purification system (Quick-gDNA MiniPrep, Zymo Research, Irvine, California). Global DNA methylation levels were quantified with a 5-methylcytosine ELISA kit according to the manufacturer's instructions (Zymo Research, Irvine, California).

Trilineage differentiation

Trilineage differentiation (AT-MSC, n = 6; BM-MSC, n = 4) was performed as previously described except where indicated [18]. Briefly, for adipogenesis and osteogenesis, cells were cultured for 14 days with either EM as described above or induction medium. Adipogenesis induction medium consisted of low-glucose DMEM with 1 μM dexamethasone (Sigma-Aldrich, St. Louis,Missouri), 0.5 mM 3-isobutyl-1-methyl-xanthine (Sigma-Aldrich, St. Louis, Missouri), 10 μg/mL recombinant human (rh) insulin (Sigma-Aldrich, St. Louis, Missouri), 0.2 mM indomethacin (Sigma-Aldrich, St. Louis, Missouri), 15% rabbit serum (Sigma-Aldrich, St. Louis, Missouri), 1% L-glutamine, and 1% antibiotic antimycotic solution (ABAM, Sigma-Aldrich, St. Louis, Missouri). Osteogenesis induction medium consisted of low-glucose DMEM with 0.1 μM dexamethasone, 10 mM glycerol 2-phosphate, 0.05 mM ascorbic acid, 10% FBS, 1% L-glutamine, and 1% ABAM. For chondrogenesis, 250,000 cells were pelleted in a 96-well plate and cultured for 21 days in high-glucose DMEM (Lonza, Walkersville, Maryland), 0.1 μM dexamethasone, 0.1 mg/mL ascorbic acid (Sigma-Aldrich, St. Louis, Missouri), 10 ng/mL TGF-β3 (R&D Systems, Minneapolis, Minnesota), 200 mM Glutamax (Life Technologies, Grand Island, New York), 10 mg proline (Sigma-Aldrich, St. Louis, Missouri), 40 μg/mL ascorbic acid, 100 mM sodium pyruvate (Life Technologies, Grand Island, New York), 1% Insulin-Transferrin-Selenium (Life Technologies, Grand Island, New York), 1% L-glutamine, and 1% ABAM. To promote better chondrogenesis, 0, 50, 100, or 200 ng/mL bone morphogenic protein 2 (BMP-2) was added to the media.

Adipogenesis and osteogenesis samples were stained with Oil Red O and Alizarin Red S stains (Sigma-Aldrich, St. Louis, Missouri) respectively. Chondrogenesis samples were histologically evaluated with toluidine blue staining for glycosaminoglycan content and hematoxylin and eosin staining for general pellet structure as previously reported [36]. Adipogenic, osteogenic, and chondrogenic mRNA transcript abundance was analyzed by RT-qPCR using the primers listed in Table 2. cDNA was synthesized from 500 ng RNA using the High Capacity cDNA Reverse Transcription Kit (Life Technologies, Grand Island, New York) using manufacturers' instructions. PCR reactions were performed using the PerfeCta SYBR Green FastMix, ROX (Quanta BioScience, Gaithersburg, Maryland) with the Applied Biosystems 7300 Real Time PCR system. Data were analyzed using the 2-ΔΔCT method. Gene expression data is presented as the induction medium-treated cultures relative to the expansion medium-treated control cultures with GAPDH used as reference gene.

Immunomodulatory properties

Whole blood was obtained from the jugular vein of dogs with an 18-gauge needle attached to a 450 mL blood collection bag (Fenwal, Baxter, Deerfield, Illinois). PBMC were isolated using a density gradient media (Ficoll-Paque Plus, GE Healthcare, Mississauga, Ontario). In a 50 mL tube, 7.5 mL of Ficoll-Paque Plus was added to the bottom. A 10 mL 1:1 mix of whole blood and PBS was then added on top and spun at 400 g for 20 min with acceleration set to 1 and deceleration set to 0. The mononuclear layers were pooled and washed repeatedly with PBS before resuspension in EM. PBMC were counted and frozen in EM with 10% DMSO (Sigma-Aldrich, St. Louis, Missouri) until use in the lymphocyte proliferation assays.

AT- and BM-MSC (AT-MSC, n = 4; BM-MSC, n = 4) were thawed and seeded 7 days prior to coculture with PBMC. On day 5, 4 treatments of each MSC were designated: 1) 200 ng/mL recombinant canine interferon-gamma (IFN-γ, Kingfisher Biotech, Saint Paul, Minnesota, Cat# RP0271D-025) added, 2) 50 ng/mL recombinant canine tumour necrosis factor-alpha (TNF-α, R&D Systems, Minneapolis, Minnesota, Cat#1507-CT-025) added, 3) both IFN-γ and TNF-α added, and 4) neither IFN-γ nor TNF-α added. Lymphocyte reaction plates (48 well) were set up on day 7. PBMC were seeded at 500,000 cells per well and stimulated with 5 μg/mL concanavalin A. MSC were irradiated with 20 Gγ and seeded at 50,000 cells per well. Corresponding MSC treatments were continued accordingly in the reaction plates. After 72 hours, 5-ethynyl-2'-deoxyuridine (EdU, a modified thymidine analogue) was added at a concentration of 10 μM and left for 24 hours before cells were collected and processed according to manufacturer's directions (Click-iT Plus EdU Flow Cytometry Assay Kit, Fisher Scientific, Ottawa, Ontario). EdU is incorporated during DNA synthesis and is used to quantify newly-synthesized DNA. Staining was completed the following day with Alexa Fluor 647 picolyl azide and analyzed using the Accuri C6 flow cytometer and software.

Data analysis

Results were modelled as multi-factor factorials in a randomized complete block design treating dog as a blocking factor. Least squares means were determined. Log transformation of data was performed where necessary and back-transformed for readability. We tested residuals for normality and plotted them against the predicted values and factors to assess ANOVA assumptions and to look for unequal variance. We found that data were normal except for outliers in the adipogenesis data, but no outliers were removed. For the gene expression data, least squares means were converted to fold-difference by using 2ΔΔCT. Data are presented as mean ± confidence interval with statistical difference assessed at P<0.05. All data analysis was performed using R statistical software (version 3.2.3, The R Foundation for Statistical Computing, Vienna, Austria).


MSC isolation

As reported [18], our criteria for isolation success was based not only on colony formation, but also the ability to expand to a minimum 5 million cells. Accordingly, 8/8 AT-MSC and only 6/8 BM-MSC met these isolation criteria.

MSC proliferation

AT-MSC proliferated faster than BM-MSC with significantly lower doubling times (P < 0.001) at all passages (P) between 2 and 5 (Fig 1). Proliferation rate also decreased with increasing passage for MSC from both cell sources as significant differences were found between both P2 and P5 (P = 0.02) and P3 and P5 (P = 0.02). Mean (± 95% confidence interval) doubling time in days were P2: (AT)1.72 ± 0.23, (BM)3.57 ± 0.23; P3: (AT)1.75 ± 0.23, (BM)3.62 ± 0.23; P4: (AT)2.30 ± 0.23, (BM)4.75 ± 0.23; P5: (AT)3.28 ± 0.23, (BM)6.77 ± 0.23.

Fig 1. Adipose tissue (AT) derived mesenchymal stromal cells (MSC) proliferate faster than those derived from bone marrow (BM).

Population doubling time of canine AT- and BM-derived MSC from passage 2 to 5. (*P<0.05, ***P<0.001; error bars = CI.)


Very similar cell surface molecule expression profiles were detected between AT- and BM-MSC (Table 3). MSC from both sources were highly positive for CD90, CD44, CD29, and MHC I while negative for CD45 and MHC II. Moderate expression of CD73, CD8 and mild expression of CD14 was also found in both cell types. The only differences seen were in the expression of CD4 (AT: moderate, BM: mild) and CD34 (AT: mild, BM: negative).

Table 3. Surface marker expression of canine adipose tissue (AT)-, bone marrow (BM)-derived mesenchymal stromal cells (MSC), and peripheral blood mononuclear cells (PBMC).

Global DNA methylation quantification

AT-MSC showed significantly higher (P<0.001) genome-wide DNA methylation levels (6.59 ± 0.52%) than BM-MSC (3.81 ± 0.30%) (Fig 2).

Fig 2. Percent 5-mC detected in genomic DNA from canine adipose- and bone marrow-derived mesenchymal stromal cells.

(***P<0.001; error bars = CI.)

Trilineage differentiation

After an induction period of 14 days, both AT- and BM-MSC stained positive for adipogenesis (Fig 3A) and osteogenesis (Fig 3B). Adipogenic mRNA transcript abundance (Fig 4) of leptin was upregulated in AT-MSC (11.15-fold, P<0.001) and BM-MSC (12.40-fold, P<0.001) and lipoprotein lipase (LPL) was upregulated in AT-MSC only (6.02-fold, P = 0.002). Osteogenic mRNA levels (Fig 5) were upregulated for osteopontin (OPN) in AT-MSC (13.21-fold, P<0.001) and BM-MSC (5.73-fold, P = 0.004) and for Runt-related transcription factor 2 (RUNX2) in AT-MSC (4.30-fold, P = 0.03) and BM-MSC (6.96-fold, P = 0.002). A significant difference was discovered (P = 0.03) between AT- and BM-MSC for alkaline phosphatase (ALP) mRNA with upregulation found only in AT-MSC (20.63-fold, P<0.001). Chondrogenesis was unsuccessful (Fig 6) after a 21 day induction period regardless of the concentration of BMP-2 added. However, AT-MSC are BMP-sensitive as noted by increased Toluidine Blue staining and more heterogeneous tissue formation compared to TGF-β3 alone as well as BMP supplemented BM-MSC.

Fig 3. Adipogenic and osteogenic induction of AT- and BM-derived canine MSC.

(A) Adipogenic potential of both canine adipose tissue (AT)- and bone marrow (BM)-derived mesenchymal stromal cells was indicated with positive Oil Red O staining after 14 days in induction medium. Control samples were negative for Oil Red O staining. Scale bars = 100 μm. (B) Osteogenic potential of both canine adipose tissue (AT)- and bone marrow (BM)-derived mesenchymal stromal cells was indicated with positive Alizarin Red S staining after 14 days in induction medium. Control samples were negative for Alizarin Red S staining. Images were adjusted for brightness and contrast. Scale bars = 200 μm.

Fig 4. Upregulation of adipogenesis markers leptin and lipoprotein lipase (LPL).

Difference in adipogenesis marker expression of canine adipose tissue- and bone marrow-derived mesenchymal stromal cells after 14 days in induction medium. (*P<0.05, **P<0.01, ***P<0.001; error bars = 95% CI.)

Fig 5. Upregulation of osteogenesis markers alkaline phosphatase (ALP), osteopontin (OPN), and Runt-related transcription factor 2 (RUNX2).

Difference in osteogenesis marker expression of canine adipose tissue- and bone marrow-derived mesenchymal stromal cells after 14 days in induction medium. (*P<0.05, **P<0.01, ***P<0.001; error bars = 95% CI.)

Fig 6. Poor chondrogenic potential of both canine adipose tissue (AT)- and bone marrow (BM)-derived mesenchymal stromal cells.

Induction time was 21 days in medium containing 10 ng/mL transforming growth factor beta 3 (TGF-β) and between 0 and 200 ng/mL bone morphogenic protein 2 (BMP-2). Samples stained with (A) hematoxylin and eosin and (B) toluidine blue. Images were adjusted for brightness and contrast. Scale bars = 100 μm.

Immunomodulatory properties

Lymphocyte proliferation assays were used to assess the lymphocyte-suppressive capacity of different canine MSC populations. AT- and BM-MSC equally suppressed stimulated PBMC proliferation when compared with stimulated PBMC alone (Fig 7). Priming the MSC with treatments of IFN-γ, TNF-α, or both had no effect on MSC immunomodulatory capacity.

Fig 7. Canine MSC inhibit T-cell proliferation.

Concanavalin A-stimulated peripheral blood mononuclear cells (PBMC) were cocultured with adipose tissue- or bone marrow-derived MSC treated with interferon-gamma, tumour necrosis factor-alpha, both, or neither. Stimulated and unstimulated PBMC were used as controls.


This is the first study to compare the immunomodulatory capacities of canine AT- and BM-MSC in addition to evaluating their general characterization and differentiation potentials. We found that both sources of MSC had proficient immunosuppressive properties. In characterizing AT- and BM-MSC, we found no profound differences between the cell types except for the significantly higher expansion rate of AT-MSC, which has been previously reported [39]. Faster proliferation along with the potential for a less invasive method of their procurement makes them the preferred source for canine MSC.

We cocultured PBMC stimulated with Con-A with irradiated AT- or BM-MSC in order to determine whether they could suppress lymphocyte proliferation. We tested MSC cultured with and without proinflammatory factors IFN-γ, TNF-α, or both for 3 days leading up to, plus the 4 days of, coculture with PBMC. While all treatment groups successfully suppressed PBMC proliferation, no treatment significantly outperformed any other within each source group (Fig 7). It is possible that a larger sample size would discern greater differences trending toward BM-MSC as PBMC proliferation is consistently lower in these wells across treatments.

If differences in immunomodulatory capacity were to emerge, the question of whether differences in surface marker expression might correlate with a more potent immunosuppressive phenotype becomes an interesting one. Our results are in agreement with the canine literature for those surface markers that show consistent expression across several studies [6,10,15,35,36,3943], in particular, positive CD90 and CD44 and negative CD45 expression. AT-MSC showed moderately higher expression of CD34 (18.6% ± 3.4) than BM-MSC (3.6% ± 1.5) and CD4 (48.0% ± 1.7 versus 19.9 ± 9.7). All other markers fell within the same ranges of expression as seen in Table 3. It has been recently reported that fat and bone marrow harvest sites do have some influence on surface marker expression [14], and likely played a role here as well.

Our first attempt at chondrogenesis of canine MSC [18] was poorly demonstrated after 21 days in the induction medium we use routinely with equine MSC [37,44]. To enhance our induction medium, we added BMP2 at different concentrations based on several reports showing it was a potent driver of MSC chondrogenesis [4549]. Unfortunately, in spite of these efforts, chondrogenesis did not improve (Fig 6). Pellets generally appeared necrotic with no evidence of lacunae formation across all samples. AT-MSC were BMP sensitive as evidence by altered pellet morphology and Toluidine Blue staining pattern. BMPs therefore remain candidates for aiding the chondrogenic differentiation, but more work is needed to determine their temporal and co-induction molecular interplays. It should be noted that canine chondrogenesis has not been robustly demonstrated in the literature as has been noted by others [10]. Until an effective induction protocol is found, it appears that in vitro MSC chondrogenic differentiation is limited in the dog compared to other species.

Adipogenic potential was demonstrated with induced cells rich with lipid droplets stained with Oil Red O (Fig 3A). Histological data was supported by gene expression analysis showing upregulation of adipogenesis markers leptin in both AT- and BM-MSC and LPL in the AT-MSC samples (Fig 4). Likewise, osteogenic potential was also demonstrated with evident mineralization stained with Alizarin Red S supported by upregulation of osteogenesis markers OPN and RUNX2 in both AT- and BM-MSC and ALP in AT-MSC. It was thought that the reduced global DNA methylation levels of BM-MSC (Fig 2) might provide the cells stronger differentiation potential [50,51]. However, at least with the three lineages induced, global DNA methylation levels had little effect. It would be interesting to examine the ability of these cells to differentiate outside the trilineage cell fates.

Ultimately, there were few differences detected between AT- and BM-MSC with regard to immunophenotyping, differentiation potential, or immunomodulatory capacity. Major differences between the sources of MSC were only found in DNA methylation levels and proliferation doubling time. This may seem counterintuitive, but this simple measure of global methylation accounts neither for specific patterns of DNA methylation nor other factors affecting gene expression like histone modification. While the difference in DNA methylation appears to have no detectable effect on differentiation potential, a higher rate of proliferation provides a key advantage to AT-MSC.

Regardless of cell source, the significant in vitro suppression of mononuclear cells warrants in vivo investigation of canine AT- and BM-MSC efficacy in modulating the immune system of inflammation-based conditions. As for their progenitor side, new protocols for chondrogenesis will need to be developed if canine MSC are to serve as chondroprogenitor cells. Failing that, other canine cells with chondrogenic potential should also be considered.

Supporting Information

S1 File. Data for proliferation (population doubling time).


S3 File. Data for global DNA methylation quantification.


S4 File. Data for adipogenesis marker gene expession.


S5 File. Data for osteogenesis marker gene expression.


S6 File. Data for lymphocyte proliferation assays.



We would like to thank Jing Zhang for her work in performing real-time PCR, Laura Furness for her help irradiating cells, and Gabrielle Monteith for guidance with statistical analysis.

Author Contributions

  1. Conceptualization: KAR TWGG JL DHB TGK.
  2. Data curation: KAR DD.
  3. Formal analysis: KAR.
  4. Funding acquisition: TWGG TGK.
  5. Investigation: KAR NHCC DD.
  6. Methodology: KAR NHCC DD TGK.
  7. Project administration: KAR TGK.
  8. Resources: TWGG TGK.
  9. Supervision: KAR TWGG TGK.
  10. Validation: KAR NHCC DD.
  11. Visualization: KAR.
  12. Writing – original draft: KAR.
  13. Writing – review & editing: KAR NHCC DD TWGG DHB TGK.


  1. 1. Uccelli A, Moretta L, Pistoia V. Mesenchymal stem cells in health and disease. Nat Rev Immunol. 2008;8(9):726–36. pmid:19172693
  2. 2. Dominici M, Le Blanc K, Mueller I, Slaper-Cortenbach I, Marini F, Krause D, et al. Minimal criteria for defining multipotent mesenchymal stromal cells. The International Society for Cellular Therapy position statement. Cytotherapy. 2006 Jan;8(4):315–7. pmid:16923606
  3. 3. de Bakker E, Van Ryssen B, De Schauwer C, Meyer E. Canine mesenchymal stem cells: state of the art, perspectives as therapy for dogs and as a model for man. Vet Q. 2014 Jan 10;2176(December 2014):1–9.
  4. 4. Bertolo A, Steffen F, Malonzo-Marty C, Stoyanov J. Canine Mesenchymal Stem Cell Potential and the Importance of Dog Breed—Implication for Cell-based Therapies. Cell Transplant. 2014 Nov 5;24(14):1969–80.
  5. 5. Choi S-A, Choi H-S, Kim KJ, Lee D-S, Lee JH, Park JY, et al. Isolation of canine mesenchymal stem cells from amniotic fluid and differentiation into hepatocyte-like cells. In Vitro Cell Dev Biol Anim. 2013 Jan;49(1):42–51. pmid:23242927
  6. 6. Csaki C, Matis U, Mobasheri A, Ye H, Shakibaei M. Chondrogenesis, osteogenesis and adipogenesis of canine mesenchymal stem cells: a biochemical, morphological and ultrastructural study. Histochem Cell Biol. 2007 Dec;128(6):507–20. pmid:17922135
  7. 7. Eslaminejad MB, Taghiyar L. Study of the Structure of Canine Mesenchymal Stem Cell Osteogenic Culture. Anat Histol Embryol. 2010;39:1–10.
  8. 8. Guercio A, Bella S Di, Casella S, Marco P Di, Russo C, Piccione G. Canine mesenchymal stemcells (mscs): Characterization in relation to donor age and adipose tissue-harvesting site. Cell Biol Int. 2013 Mar 15;37(8):789–98. pmid:23505013
  9. 9. Hodgkiss-Geere HM, Argyle DJ, Corcoran BM, Whitelaw B, Milne E, Bennett D, et al. Characterisation and differentiation potential of bone marrow derived canine mesenchymal stem cells. Vet J. 2012 Jun 19;194(3):361–8. pmid:22721628
  10. 10. Kisiel AH, McDuffee L a, Masaoud E, Bailey TR, Esparza Gonzalez BP, Nino-Fong R. Isolation, characterization, and in vitro proliferation of canine mesenchymal stem cells derived from bone marrow, adipose tissue, muscle, and periosteum. Am J Vet Res. 2012 Aug;73(8):1305–17. pmid:22849692
  11. 11. Lee J, Byeon JS, Lee KS, Gu N-YY, Lee GB, Kim H-RR, et al. Chondrogenic potential and anti-senescence effect of hypoxia on canine adipose mesenchymal stem cells. Vet Res Commun. 2015;1–10.
  12. 12. Neupane M, Chang C-C, Kiupel M, Yuzbasiyan-Gurkan V. Isolation and characterization of canine adipose-derived mesenchymal stem cells. Tissue Eng Part A. 2008 Jun;14(6):1007–15. pmid:19230125
  13. 13. Reich CM, Raabe O, Wenisch S, Bridger PS, Kramer M, Arnhold S. Isolation, culture and chondrogenic differentiation of canine adipose tissue- and bone marrow-derived mesenchymal stem cells-a comparative study. Vet Res Commun. 2012 Mar 4;139–48. pmid:22392598
  14. 14. Sullivan MO, Gordon-Evans WJ, Fredericks LP, Kiefer K, Conzemius MG, Griffon DJ. Comparison of Mesenchymal Stem Cell Surface Markers from Bone Marrow Aspirates and Adipose Stromal Vascular Fraction Sites. Front Vet Sci. 2016;2(January):1–9.
  15. 15. Vieira NM, Brandalise V, Zucconi E, Secco M, Strauss BE, Zatz M. Isolation, characterization, and differentiation potential of canine adipose-derived stem cells. Cell Transplant. 2010 Jan;19(3):279–89. pmid:19995482
  16. 16. Volk SW, Wang Y, Hankenson KD. Effects of donor characteristics and ex vivo expansion on canine mesenchymal stem cell properties: Implications for MSC-based therapies. Cell Transplant. 2012 Apr 2;21(10):2189–200. pmid:22472645
  17. 17. Zucconi E, Vieira NM, Bueno DF, Secco M, Jazedje T, Ambrosio CE, et al. Mesenchymal stem cells derived from canine umbilical cord vein—a novel source for cell therapy studies. Stem Cells Dev. 2010 Mar;19(3):395–402. pmid:19290805
  18. 18. Russell KA, Gibson TWG, Chong A, Co C, Koch TG. Canine Platelet Lysate Is Inferior to Fetal Bovine Serum for the Isolation and Propagation of Canine Adipose Tissue- and Bone Marrow-Derived Mesenchymal Stromal Cells. PLoS One. 2015;10(9):1–14.
  19. 19. Meirelles LDS, Fontes AM, Covas DT, Caplan AI. Mechanisms involved in the therapeutic properties of mesenchymal stem cells. Cytokine Growth Factor Rev. 2009;20(5–6):419–27. pmid:19926330
  20. 20. Griffin MD, Ritter T, Mahon BP. Immunological aspects of allogeneic mesenchymal stem cell therapies. Hum Gene Ther. 2010;21(12):1641–55. pmid:20718666
  21. 21. Bartholomew A, Sturgeon C, Siatskas M, Ferrer K, Mcintosh K, Patil S, et al. Mesenchymal stem cells suppress lymphocyte proliferation in vitro and prolong skin graft survival in vivo. Hematology. 2002;30:42–8.
  22. 22. Di Nicola M. Human bone marrow stromal cells suppress T-lymphocyte proliferation induced by cellular or nonspecific mitogenic stimuli. Blood. 2002 May 15;99(10):3838–43. pmid:11986244
  23. 23. Puissant B, Barreau C, Bourin P, Clavel C, Corre J, Bousquet C, et al. Immunomodulatory effect of human adipose tissue-derived adult stem cells: comparison with bone marrow mesenchymal stem cells. Br J Haematol. 2005 Apr;129(1):118–29. pmid:15801964
  24. 24. Le Blanc K, Mougiakakos D. Multipotent mesenchymal stromal cells and the innate immune system. Nat Rev Immunol. 2012;12(5):383–96. pmid:22531326
  25. 25. Yagi H, Soto-gutierrez A, Parekkadan B, Kitagawa Y, Tompkins G, Kobayashi N, et al. Mesenchymal Stem Cells: Mechanisms of Immunomodulation and Homing. Cell Transplant. 2010;19(6):667–79. pmid:20525442
  26. 26. Nauta A, Fibbe W. Immunomodulatory properties of mesenchymal stromal cells. Blood. 2007;110(10):3499–506. pmid:17664353
  27. 27. Krampera M, Cosmi L, Angeli R, Pasini A, Liotta F, Andreini A, et al. Role for Interferon-γ in the Immunomodulatory Activity of Human Bone Marrow Mesenchymal Stem Cells. Stem Cells. 2006;24(2):386–98. pmid:16123384
  28. 28. Ren G, Zhang L, Zhao X, Xu G, Zhang Y, Roberts AI, et al. Mesenchymal stem cell-mediated immunosuppression occurs via concerted action of chemokines and nitric oxide. Cell Stem Cell. 2008 Feb 7;2(2):141–50. pmid:18371435
  29. 29. Meisel R, Zibert A, Laryea M, Göbel U, Däubener W, Dilloo D. Human bone marrow stromal cells inhibit allogeneic T-cell responses by indoleamine 2,3-dioxygenase-mediated tryptophan degradation. Blood. 2004 Jun 15;103(12):4619–21. pmid:15001472
  30. 30. English K, Barry FP, Field-Corbett CP, Mahon BP. IFN-γ and TNF-α differentially regulate immunomodulation by murine mesenchymal stem cells. Immunol Lett. 2007;110(2):91–100. pmid:17507101
  31. 31. Ryan JM, Barry F, Murphy JM, Mahon BP. Interferon-gamma does not break, but promotes the immunosuppressive capacity of adult human mesenchymal stem cells. Clin Exp Immunol. 2007 Aug;149(2):353–63. pmid:17521318
  32. 32. Kol A, Foutouhi S, Walker NJ, Kong NT, Weimer BC, Borjesson DL. Gastrointestinal microbes interact with canine adipose-derived mesenchymal stem cells in vitro and enhance immunomodulatory functions. Stem Cells Dev. 2014;23(16):1831–43. pmid:24803072
  33. 33. Park SA, Reilly CM, Wood J a., Chung DJ, Carrade DD, Deremer SL, et al. Safety and immunomodulatory effects of allogeneic canine adipose-derived mesenchymal stromal cells transplanted into the region of the lacrimal gland, the gland of the third eyelid and the knee joint. Cytotherapy. 2013;15(12):1498–510. pmid:23992828
  34. 34. Lee WS, Suzuki Y, Graves SS, Iwata M, Venkataraman GM, Mielcarek M, et al. Canine bone marrow-derived mesenchymal stromal cells suppress alloreactive lymphocyte proliferation in vitro but fail to enhance engraftment in canine bone marrow transplantation. Biol Blood Marrow Transplant. 2011 Apr;17(4):465–75. pmid:20457265
  35. 35. Kang JW, Kang K-S, Koo HC, Park JR, Choi EW, Park YH. Soluble factors-mediated immunomodulatory effects of canine adipose tissue-derived mesenchymal stem cells. Stem Cells Dev. 2008 Aug;17(4):681–93. pmid:18717642
  36. 36. Co C, Vickaryous MK, Koch TG. Membrane culture and reduced oxygen tension enhances cartilage matrix formation from equine cord blood mesenchymal stromal cells invitro. Osteoarthr Cartil. 2014 Jan 11;22:472–80. pmid:24418676
  37. 37. Figueroa RJ, Koch TG, Betts DH. Osteogenic differentiation of equine cord blood multipotent mesenchymal stromal cells within coralline hydroxyapatite scaffolds in vitro. Vet Comp Orthop Traumatol. 2011 Jan;24(5):354–62. pmid:21792475
  38. 38. Brinkhof B, Spee B, Rothuizen J, Penning LC. Development and evaluation of canine reference genes for accurate quantification of gene expression. Anal Biochem. 2006 Sep 1;356(1):36–43. pmid:16844072
  39. 39. Kang BJ, Ryu HH, Park SS, Koyama Y, Kikuchi M, Woo HM, et al. Comparing the osteogenic potential of canine mesenchymal stem cells derived from adipose tissues, bone marrow, umbilical cord blood, and Wharton’s jelly for treating bone defects. J Vet Sci. 2012;13(3):299–310. pmid:23000587
  40. 40. 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 Jan;8(1):150.
  41. 41. Martinello T, Bronzini I, Maccatrozzo L, Mollo a, Sampaolesi M, Mascarello F, et al. Canine adipose-derived-mesenchymal stem cells do not lose stem features after a long-term cryopreservation. Res Vet Sci. 2011 Aug;91(1):18–24. pmid:20732703
  42. 42. Kamishina H, Deng J, Oji T, Cheeseman J a, Clemmons RM. Expression of neural markers on bone marrow-derived canine mesenchymal stem cells. Am J Vet Res. 2006 Nov;67(11):1921–8. pmid:17078756
  43. 43. Screven R, Kenyon E, Myers MJ, Yancy HF, Skasko M, Boxer L, et al. Immunophenotype and gene expression profiles of mesenchymal stem cells derived from canine adipose tissue and bone marrow. Vet Immunol Immunopathol. 2014;161(1–2):21–31. pmid:25026887
  44. 44. Berg L, Koch T, Heerkens T, Bessonov K, Thomsen P, Betts D. Chondrogenic potential of mesenchymal stromal cells derived from equine bone marrow and umbilical cord blood. Vet Comp Orthop Traumatol. 2009 Jan;22(5):363–70. pmid:19750290
  45. 45. Schmitt B, Ringe J, Häupl T, Notter M, Manz R, Burmester GR, et al. BMP2 initiates chondrogenic lineage development of adult human mesenchymal stem cells in high-density culture. Differentiation. 2003;71(9–10):567–77. pmid:14686954
  46. 46. Guilak F, Awad H a, Fermor B, Leddy H a, Gimble JM. Adipose-derived adult stem cells for cartilage tissue engineering. Biorheology. 2004 Jan;41(3–4):389–99. pmid:15299271
  47. 47. Toh WS, Liu H, Heng BC, Rufaihah AJ, Ye CP, Cao T. Combined effects of TGFbeta1 and BMP2 in serum-free chondrogenic differentiation of mesenchymal stem cells induced hyaline-like cartilage formation. Growth Factors. 2005 Dec;23(4):313–21. pmid:16338794
  48. 48. Shirasawa S, Sekiya I, Sakaguchi Y, Yagishita K, Ichinose S, Muneta T. In vitro chondrogenesis of human synovium-derived mesenchymal stem cells: Optimal condition and comparison with bone marrow-derived cells. J Cell Biochem. 2006;97(1):84–97. pmid:16088956
  49. 49. An C, Cheng Y, Yuan Q, Li J. IGF-1 and BMP-2 induces differentiation of adipose-derived mesenchymal stem cells into chondrocytes-like cells. Ann Biomed Eng. 2010;38(4):1647–54. pmid:20052615
  50. 50. Collas P, Noer A, Sørensen AL. Epigenetic basis for the differentiation potential of mesenchymal and embryonic stem cells. Transfus Med Hemotherapy. 2008;35(3):205–15.
  51. 51. Berdasco M, Esteller M. DNA methylation in stem cell renewal and multipotency. Stem Cell Res Ther. 2011;2(5):42. pmid:22041459