Functional characterization of the immunomodulatory properties of human urine-derived stem cells.

BACKGROUND: Urine-derived stem cells (USCs) have been widely researched as a novel cell source for stem cell therapy, but their immunomodulatory characteristics remain to be investigated. This study aimed to characterize the immunomodulatory properties of human USCs.
METHODS: Human USCs were isolated from fresh voiding urine samples from healthy male donors and expanded. Their cell surface markers were characterized by flow cytometry analysis and the telomerase activities for several USCs clones were determined. The immunosuppressive potential of USCs was evaluated by the performing the mixed lymphocyte reaction (MLR) [co-culture with peripheral blood mononuclear cells (PBMNCs)] and natural killer cells (NK) cytotoxicity assay. USCs cytokines release profile was determined by using human cytokine proteome array.
RESULTS: USCs exhibited high cell surface expression of embryonic/mesenchymal stem cells (MSCs) markers CD29, CD44, CD54, CD73, CD90, CD146, and CD166, while lacked expression of hematopoietic stem cell markers CD11, CD14, CD19, CD31, CD34, CD45, B cell marker CD79, and co-stimulatory factors CD80 and CD86, thus, exhibiting the phenotype of MSCs. MLR indicated that USCs significantly inhibited the proliferation of PBMNCs, as compared to that of the human smooth muscle cells (SMCs). In cell cytotoxicity assays, NK cells displayed less cytotoxicity against USCs than against bone marrow mesenchymal stem cells (BMSCs) and SMCs. Furthermore, upon PBMNCs stimulation, USCs secreted higher levels of immunomodulatory cytokines, including IL-6, IL-8, MCP-1, RANTES, GROα, and GM-CSF, compared to those of BMSCs, especially when directly contact mix-culture with PBMNCs.
CONCLUSIONS: USCs secreted immunoregulatory cytokines and possessed immunomodulatory properties, comparable to those of BMSCs. 2021 Translational Andrology and Urology. All rights reserved.

Introduction

Immune-mediated diseases are one of the largest types of diseases clinically studied. Autoimmune diseases are pathological states in which the immune system exerts abnormal cellular or antibody responses against patient’s own tissues and organs, leading to chronic inflammation (1). These diseases affect more than 5% of the worldwide population, seriously impacting on the patient’s quality of life and health care costs (2). Autoimmune diseases induce both local and systemic symptoms, leading to severe outcomes, such as systemic lupus erythematosus, rheumatoid arthritis, multiple sclerosis, and type I diabetes (2). Currently autoimmune diseases are generally treated with immune suppressive agents, such as steroids and cyclosporine. However, prolonged use of these medicines has been shown to increase treatment-related morbidity and mortality (3). Thus, development of new therapeutic strategies for autoimmune diseases is urgently required.

Stem cell therapy has been demonstrated to possess the capacity to modulate the immune system and reduce the severity of the disease in animal models of autoimmune disorders (4). For instance, rheumatoid arthritis (5), multiple sclerosis (6), lupus (7), inflammatory bowel diseases (8), among other autoimmune diseases, have responded to stem cell therapy both in preclinical and clinical studies. Among all types of stem cells, mesenchymal stem cells (MSCs) are commonly used for cell therapy due to their profound immunomodulatory properties and differentiation potentials (9), to most importantly regenerate and repair tissue. MSCs are capable of differentiating into cells of the mesodermal, endodermal, and even ectodermal lineages. Furthermore, increased evidence has shown that under appropriate culture conditions, MSCs are capable of secreting growth factors and immunoprotective cytokines, used in the field of cell and organ transplantation. Importantly, MSCs are safe and do not form teratoma, compared to embryonic or induced pluripotent stem cells.

In addition, MSCs are hypoimmunogenic and can escape the recognition by all-reactive T cells and natural killer (NK) cells and their subsequent cytotoxicities (9). These cells are capable of inhibiting the proliferation and activity of immune effector cells, thereby ameliorating the severity of the immune disease (9). Since first identified in the bone marrow (10), MSCs have been isolated from various tissues, called tissue-derived stem cells. The most commonly used types of MSCs in preclinical and clinical studies are cells originated from the bone marrow (BMSCs) (11), umbilical cord (UC-MSCs) (12), and adipose tissue (ADSCs) (13). Although both BMSCs and ADSCs have been investigated for a long period and applied in various experimental studies and preclinical trials (14), harvesting ADSCs and BMSCs requires invasive medical procedures, which could cause potential complications and even risk to the donor’s lives. The ideal MSCs cell source should be less invasive and harmful to the donor, as well as ease to harvest and expand in large quantities. Considering this requirement, in 2008, Zhang et al. first demonstrated that stem cells can be isolated from fresh urine sample (15), termed as urine-derived stem cells (USCs). These cells have similar characteristics to MSCs (11,16), can be efficiently induced into ectodermal, mesodermal, and endodermal lineages. Despite a few cells have a “rice-grain-like” morphology in the urine, they can consecutively proliferate up to 20 passages, with a doubling rate of more than 60 (16). These cells most likely originate from the parietal cell interface of the renal glomerulus and express the corresponding markers (16). More than half of USCs clones possess high telomerase activity and proliferation ability; large quantities can be obtained from a single cell (3,17). Importantly, USCs can be isolated from fresh voiding urine and propagated through a simple, noninvasive, and low-cost manipulation, making them more attractive for tissue regeneration.

Therefore, USCs can be a novel alternative cell source for stem cell therapy (18). However, the immunomodulatory properties of USCs have not been fully investigated thus far. Hence, the purpose of this study was to characterize the immunomodulatory properties of human USCs.

We present the following article in accordance with the MDAR reporting checklist (available at https://dx.doi.org/10.21037/tau-21-506).

Methods

Ethics statements

This study was approved by the Wake Forest University institutional review board (IRB00014033). Written informed consents have been obtained and were approved by Wake Forest University institutional review board. The study was conducted in accordance with the Declaration of Helsinki (as revised in 2013).

Isolation of human USCs

Fresh voiding urine samples were collected from three healthy male donors of 28-, 35-, and 41-year-old, respectively. For isolation of USCs, the urine samples were centrifuged at 500 ×g for 5 min at room temperature. The cell pellets were re-suspended and then seeded into 24-well tissue culture plates (Becton Dickinson, Franklin Lakes, NJ, USA). The culture medium contained Keratinocyte Serum Free Medium (KSFM, Gibco, Gaithersburg, MD, USA) and Dulbecco’s Modified Eagle Medium (DMEM, high glucose, Gibco, Gaithersburg, MD, USA) at a 1:1 ratio with 5% fetal bovine serum (FBS, Gibco, Gaithersburg, MD, USA). Urine-derived cells were isolated and characterized as previously described (16). USCs at passages 2–5 were used for following studies.

Cell culture

Human peripheral blood mononuclear cells (PBMNCs, normal human, ATCC PCS-800-011) from two different donors were purchased from ATCC (American Type Culture Collection, MD, USA). PBMNCs were thaw in the Hank’s Balanced Salt Solution medium (HBSS, ATCC 302213, MD, USA) and directly used in the experiments. Human BMSCs and human SMCs were purchased from Lonza (BMSCs: PT-2501, SMCs: CC-2533, Lonza, Swiss).

Flow cytometry for stem cell surface markers

USCs at passage 2 were stained with specific antibodies against human CD11b-FITC, CD14-APC, CD19-FITC, CD29-PE, CD31-FITC, CD34-FITC, CD40-FITC, CD44-FITC, CD45-FITC, CD54-PE, CD73-PE, CD79-PE, CD90-FITC, CD133-PE, CD140b-PE, CD146-PE, CD166-PE, CD80-FITC, CD86-PE, HLA-ABC-FITC, HLA-G-FITC, and HLA-DR-FITC. Briefly, cells were trypsinized and a total of 5.0×105 cells were re-suspended in ice-cold PBS containing 1% bovine serum albumin (BSA, 23210, Thermo Fisher scientific, Rockford, IL, USA). Fluorochrome-conjugated antibodies () were added to 50 µL of the cell suspension containing 1×PBS and 1% BSA, the mix was incubated on ice for 30 min in the dark. IgG1-PE, IgG1-FITC, IgG2b-FITC, and IgG1-APC conjugated isotype control antibodies were used to determine the background fluorescence. Cells were then washed twice in wash buffer, passed through a 70 µm filter, and detected by flow cytometry (FACS Calibur BD Biosciences, Franklin Lakes, NJ, USA), procedures were repeated three times. The data were analyzed by using FlowJo vX software (Tree Star, Ashland, OR, USA).

Table 1

Antibodies used in this study

Antibody	Type	Dilution	Source (company)	Catalog No.
CD11b-FITC	Mouse mAb	1:10	BD Pharmingen™	562793
CD14-APC	Mouse mAb	1:10	BD Pharmingen™	561708
CD19-FITC	Mouse mAb	1:10	BD Pharmingen™	560994
CD29-PE	Mouse mAb	1:10	BD Pharmingen™	555443
CD31-FITC	Mouse mAb	1:10	BD Pharmingen™	560984
CD34-FITC	Mouse mAb	1:10	BD Pharmingen™	560942
CD40-FITC	Mouse mAb	1:10	BD Pharmingen™	556624
CD44-FITC	Mouse mAb	1:10	BD Pharmingen™	555478
CD45-FITC	Mouse mAb	1:10	BD Pharmingen™	560976
CD54-PE	Mouse mAb	1:10	BD Pharmingen™	560971
CD73-PE	Mouse mAb	1:10	BD Pharmingen™	561014
CD79-PE	Mouse mAb	1:10	BD Pharmingen™	563777
CD90-FITC	Mouse mAb	1:10	BD Pharmingen™	555595
CD140b-PE	Mouse mAb	1:10	BD Pharmingen™	558821
CD146-PE	Mouse mAb	1:10	BD Pharmingen™	550315
CD166-PE	Mouse mAb	1:10	BD Pharmingen™	560903
CD80-FITC	Mouse mAb	1:10	BD Pharmingen™	557226
CD86-PE	Mouse mAb	1:10	BD Pharmingen™	557344
HLA-ABC-FITC	Mouse mAb	1:10	BD Pharmingen™	555552
HLA-G-FITC	Mouse mAb	1:10	BD Pharmingen™	557577
HLA-DR-FITC	Mouse mAb	1:10	BD Pharmingen™	562008

Telomerase activity assay

The telomerase activity of USCs was directly associated with their proliferative potential according to our prior research (16). Otherwise, does immune characters associate with telomerase activity not clear yet. The telomerase activities of the USCs clones were determined by the telomeric repeat amplification protocol assay, using the Telo TAGGG Telomerase PCR ELISAplus kit (Roche, Germany) and according to manufacturer’s protocol. To ensure that each USCs clone was originated from a single cell, only wells in multi-well plates with a single spindle shape cell were selected for expansion. The telomerase activity of human BMSCs and SMCs, as well as of HEK293 cell line (ATCC CRL-1573, MD, USA) as control, were also measured. A total of 2×105 cells at passage 2 were collected for DNA extraction.

After DNA amplification by PCR, the products were subjected to hybridization and ELISA procedures. The results were reported by subtracting the absorbance of the samples at 450 nm. The level of telomerase activity in a given sample was determined by comparing the signal originated by the sample to the signal obtained using a known amount of a control template in the kit. Relative telomerase activities (RTA) of samples were obtained using the following formula:

RTA: relative telomerase activity; AS: absorbance of sample; AHt: absorbance of heat-treated sample; AIs: absorbance of internal standard of the sample; AC: absorbance of control template; ALb: absorbance of lysis buffer; AIsC: absorbance of internal standard of the control template. Internal standard and control template were all provided in the kit.

Mixed lymphocyte reaction (MLR)

USC-TA+ (USCs clone with high telomerase activity), USC-TA− (USCs clone with low telomerase activity), BMSCs, and SMCs were used as stimulator cells; meanwhile, human PBMNCs from two healthy donors with different blood types were used as responder cells. Approximately 1×104 stimulator cells of each type were seeded in triplicate into a 96-well flat-bottom plate (BD Falcon, USA) with Mesenchymal Stem Cell Growth Medium (MSCGM, Thermo Fisher Scientific-Gibco, Carlsbad, CA, USA). The cells were cultured to near confluency, and then treated with 5 µg/mL mitomycin C (Roche Applied Science, Mannheim, Germany) at 37 °C for 2.5 h in a humidified incubator with 5% CO2 to prevent further proliferation. After incubation, cells were washed three times with DMEM. For co-culture experiments, 1×105 responder cells were added to each well, in a final volume of 100 µL of DMEM with 10% FBS. Cultures were incubated at 37 °C for 5 days in 5% CO2 and 100% humidity and checked with inverted microscope before further experiment. On the fifth day, 10 µL of Bromodeoxyuridine (BrdU, Roche Applied Science, Mannheim, Germany) was added to each well to a final concentration of 10 µM. After incubation for additional 24 h at 37 °C in 5% CO2 and 100% humidity, DNA synthesis was assessed with the BrdU cell proliferation colorimetric ELISA Kit (Roche Applied Science, Mannheim, Germany), according to the manufacturer’s instructions. Newly synthesized BrdU-DNA was quantified using a scanning multi-well spectrophotometer (Bio-Rad, Hercules, CA, USA). One-way MLR with single donor PBMNCs as responder cells, and two-way MLR with aliquot half dose of two different donors’ PBMNCs as responder cells were detected in the same multi-well plate, respectively. All the reactions were set up in triplicate per experiment and the experiment was repeated 3 times.

NK cytotoxicity assay

Human NK-92 MI cells were purchased from ATCC (ATCC CRL-2408, MD, USA). The NK cytotoxicity assay was performed using the CytoTox96® Non-Radioactive Cytotoxicity Assay kit (Promega, WI, USA), according to the manufacturer’s protocol. 50 μL USC-TA+, USC-TA−, BMSCs, and SMCs in α-MEM complete medium without phenol red (Gibco, Gaithersburg, MD, USA) at the concentration of 1×105 cells/mL were added into a round-bottom 96-well tissue culture microplate (BD Falcon, USA) as target cells, NK-92 MI cells (effectors) at E:T ratios of 20:1, 10:1, 5:1, and 1:1 were added in the wells of target cells with the final volume of 100 μL. The plate was centrifuged at 250 ×g for 4 min, followed by incubation at 37 °C, 5% CO2 for 4 h. The plate was then centrifuged at 250 ×g for 4 min, 50 μL of each supernatant was transferred to another flat-bottom 96-well microplate containing 50 μL of substrate mix (CytoTox96® Reagent), and the microplate was incubated for 30 min at room temperature in the dark. Absorbance at 490 nm was determined using scanning multi-well spectrophotometer (Bio-Rad, Hercules, CA, USA) immediately after adding 50 μL of Stop Solution. The percentage of cell lysis was calculated based on the following equation:

Spontaneous release corresponded to the cytotoxicity of target cells alone in the medium, while target cell maximum release was obtained by adding 10 μL of 9% Triton X-100 solution to the cells and incubating the mix for 45 min at 37 °C, prior to harvesting the supernatants. All the reactions were performed in triplicate per experiment and each experiment was repeated 3 times.

Cytokine proteome array

USC-TA+, USC-TA−, BMSCs were cultured alone, cultured in direct contacting with PBMNCs, and with PBMNCs in 0.4 μm Millicell hanging cell culture transwell insert (Millipore, USA), respectively, to determine the cytokines and chemokines released by the cells. The levels of cytokines and chemokines were tested in cell culture supernatants using the Human Cytokine Array Panel A kit (R&D Systems Inc., MN, USA), according to the manufacturer’s instructions. The array panel template is showed in . Aliquot of 1 mL from each supernatant was incubated with 15 µL of human cytokine antibody cocktail for 1 h at room temperature, and the mixture was then added to previously blocked nitrocellulose membranes and incubated at 4 °C overnight on a rocking platform shaker. On the next day, the membranes were washed three times (10 min each) with 1× wash buffer and incubated with Streptavidin-HRP and Chemi Reagent Mix for 30 min at room temperature on a rocking platform shaker. The immunoblot images were visualized and captured using the LAS-3000 Image Analyzer (Fujifilm, Japan). Quantity One software (Bio-Rad, CA, USA, RRID:SCR_014280) was used to quantify the cytokine levels.

Table 2

Human cytokine array panel a coordinates

Coordinate	Target/control	Alternate nomenclature
A1, A2	Reference Spot	–
A3, A4	C5/C5a	Complement Component 5/5a
A5, A6	CD40 ligand	CD154
A7, A8	G-CSF	CSFβ, CSF-3
A9, A10	GM-CSF	CSFα, CSF-2
A11, A12	GROα	CXCL1
A13, A14	I-309	CCL1
A15, A16	sICAM-1	CD54
A17, A18	IFN-γ	Type II IFN
A19, A20	Reference Spot	–
B3, B4	IL-1α	IL-1F1
B5, B6	IL-1β	IL-1F2
B7, B8	IL-1ra	IL-1F3
B9, B10	IL-2	–
B11, B12	IL-4	–
B13, B14	IL-5	–
B15, B16	IL-6	–
B17, B18	IL-8	CXCL8
C3, C4	IL-10	–
C5, C6	IL-12 p70	–
C7, C8	IL-13	–
C9, C10	IL-16	LCF
C11, C12	IL-17	–
C13, C14	IL-17E	–
C15, C16	IL-23	–
C17, C18	IL-27	–
D3, D4	IL-32α	–
D5, D6	IP-10	CXCL10
D7, D8	I-TAC	CXCL11
D9, D10	MCP-1	CCL2
D11, D12	MIF	GIF, DER6
D13, D14	MIP-1α	CCL3
D15, D16	MIP-1β	CCL4
D17, D18	Serpin E1	PAI-1
E1, E2	Reference Spot	–
E3, E4	RANTES	CCL5
E5, E6	SDF-1	CXCL12
E7, E8	TNF-α	TNFSF1A
E9, E10	sTREM-1	–
E19, E20	Negative control	–

Statistical analysis

Data are expressed as the mean ± standard deviation (SD). Means among groups were compared by one-way ANOVA or Kruskal-Walis test (if appropriate) and the corresponding post-hoc test (Fisher’s LSD test for ANOVA). The significance level was set at P value <0.05 for all tests. Statistical analyses were performed using the SPSS software version 25 (IBM Corporation, NY, USA).

Results

USCs expressed embryonic/MSCs markers

We determined the cell markers present on the surface of isolated USCs by flow cytometry analysis (). According to our results, the USCs major population expressed typical embryonic/MSCs markers, such as CD29 (100%), CD44 (100%), CD54 (98.9%), CD73 (99.6%), CD90 (75.5%), CD146 (99.2%), and CD166 (99.4%); meanwhile, a small population of USCs expressed CD140 (10.7%). In contrast, USCs did not present hematopoietic stem cell markers CD11b (0.98%), CD14 (1.55%), CD19 (0.914%), CD31 (0.861%), CD34 (1.02%), CD45 (0.737%), and B cell marker CD79 (1.05%) on their surfaces.

Table 3

Flow cytometry for cell surface markers of USCs

Markers	Function	Flow cytometry results
CD11b	Implicated in the various adhesive interactions of monocytes, macrophages, and granulocytes	0.98%
CD14	Mediates the innate immune response to bacterial LPS	1.55%
CD19	Assembles with the antigen receptor of B lymphocytes to decrease the threshold for antigen receptor-dependent stimulation	0.914%
CD29	Cell adhesion	100%
CD31	Cell adhesion, activation, and migration	0.861%
CD34	Cell adhesion	1.02%
CD40	Cell adhesion, cell proliferation, and signal transduction	28.3%
CD44	Cell adhesion and migration	100%
CD45	Regulator of T- and B-cell antigen receptor signaling; regulator of cell growth and differentiation	0.737%
CD54	Cell adhesion, lymphocyte activation, and migration	98.9%
CD73	An ecto-5-prime-nucleotidase hydrolyzing extracellular nucleotides into membrane-permeable nucleosides	99.6%
CD79	Required for imitation of B cell signal transduction upon binding of antigen to the B-cell antigen receptor complex	1.05%
CD90	Cell adhesion	75.5%
CD140b	Tyrosine kinase receptor which binds PDGF B and D	10.7%
CD146	Cell adhesion	99.2%
CD166	Cell adhesion molecule important for intrathymic T-cell development	99.4%
CD80	Lymphocyte activation	0.86%
CD86	Costimulatory signal for T-cell activation	0.63%
HLA-ABC	The major histocompatibility complex, Class-I	99.8%
HLA-G	The major histocompatibility complex, Class-I	0.996%
HLA-DR	The major histocompatibility complex, Class-II	0.642%

LPS, lipopolysaccharide; PDGF, platelet derived growth factor.

In addition, USCs tested lightly positive for the co-stimulatory factor CD40 (28.3%) and negative for co-stimulatory factors CD80 (0.86%) and CD86 (0.63%). Regarding major histocompatibility complex (MHC) antigens, most of USCs contained HLA-ABC markers (99.8%) but the cell surface expression of HLA-DR (0.642%) and HLA-G (0.996%) antigens was negligible (). These data suggested that the isolated USCs indeed expressed MSCs markers, indicating they may possess MSCs characteristics.

Figure 1

USCs surface markers were determined by flow cytometry. Flow data showed the detection of co-stimulatory molecules CD40, CD80, and CD86 and immunological markers HLA-ABC, HLA-G, and HLA-DR.

USCs presented varied telomerase activity

After determining the telomerase activity of the USCs samples, specific clones were selected from three donors (2 clones/donor). Each donor provided two USCs clones, one with high telomerase activity (USC-TA+) and another one with low telomerase activity (USC-TA−), that were used for further studies.

USCs inhibited the proliferation of PBMNCs in MLR

To determine whether USCs had immunomodulatory properties, USC-TA+ and USC-TA− were co-cultured with PBMNCs from two different donors (one-way MLR and two-way MLR) by analyzing their immunosuppressive potentials towards PBMNCs. As shown in , both USC-TA+ and USC-TA− elicited a higher inhibition on the MLR reactions, when compared to SMCs and BMSCs, although the difference between USC-TA+, USC-TA− and BMSCs was not significant. The difference between USC-TA+/USC-TA− and SMCs was significant when using the PBMNCs no matter from one specific donor or two different donors (all P<0.05). That reveal both USC-TA+ and USC-TA− had a higher capacity to inhibit the proliferation of PBMNCs, when compared to that of SMCs control. These results suggested that both USC-TA+ and USC-TA− possessed comparable immunosuppressive potentials to that of BMSCs.

Figure 2

USCs inhibited the proliferation of PBMNCs in MLR. USC-TA+, USC-TA−, BMSCs, and SMCs were used as stimulator cells and human PBMNCs from two healthy donors were used as responder cells. One-way MLR with single donor PBMNCs (donor A or B) as responder cells and two-way MLR with aliquot half dose of two different donors’ PBMNCs (donor A and B) as responder cells were detected in the same multi-well plate. Cultures were incubated at 37 °C for 5 days in 5% CO2 and 100% humidity, the cells were checked with inverted microscope on the 5th day before further experiment. There were different cell densities of PBMNCs be noticed in different wells for 5 days mix-culture, Scale bar =50 µm (A). The proliferation of PBMNCs was assessed with the BrdU cell proliferation colorimetric ELISA. Newly synthesized BrdU-DNA was quantified using a scanning multi-well spectrophotometer (B). *, P<0.05, post-hoc paired-comparisons. MLR, mixed lymphocyte reaction; BMSC, human bone marrow mesenchymal stem cells; SMC, human smooth muscle cells; USC TA+, human urine derived stem cells with high telomerase activity; USC TA−, human urine derived stem cells with low telomerase activity; PBMNC, human peripheral blood mononuclear cells; SMC + PBMNC A, one-way mixed lymphocyte reaction as human smooth muscle cells mixed with human peripheral blood mononuclear cells from donor A; SMC + PBMNC B, one-way mixed lymphocyte reaction as human smooth muscle cells mixed with human peripheral blood mononuclear cells from donor B; SMC + PBMNC A + B, two-way mixed lymphocyte reaction as human smooth muscle cells mixed with aliquot half dose of two different donors’ human peripheral blood mononuclear cells from donor A and donor B; BMSC + PBMNC A, one-way mixed lymphocyte reaction as human bone marrow mesenchymal stem cells mixed with human peripheral blood mononuclear cells from donor A; BMSC + PBMNC B, one-way mixed lymphocyte reaction as human bone marrow mesenchymal stem cells mixed with human peripheral blood mononuclear cells from donor B; BMSC + PBMNC A + B, two-way mixed lymphocyte reaction as human bone marrow mesenchymal stem cells mixed with aliquot half dose of two different donors’ human peripheral blood mononuclear cells from donor A and donor B; USC + PBMNC A, one-way mixed lymphocyte reaction as human urine derived stem cells mixed with human peripheral blood mononuclear cells from donor A; USC + PBMNC B, one-way mixed lymphocyte reaction as human urine derived stem cells mixed with human peripheral blood mononuclear cells from donor B; USC + PBMNC A + B, two-way mixed lymphocyte reaction as human urine derived stem cells mixed with aliquot half dose of two different donors’ human peripheral blood mononuclear cells from donor A and donor B.

USCs inhibited NK cytotoxicities

Next, we further evaluated the immunomodulatory properties of USCs with NK cytotoxicity assays. The results showed that both USC-TA+ and USC-TA− induced less cytotoxicity than SMCs at E:T ratios of 20:1, 10:1, 5:1, and 1:1, although only the difference between USC-TA+ and BMSCs at the E:T ratio 10:1 was significant (P=0.013). These results suggested that USCs possessed a comparable or even a little better immunomodulatory property than that of BMSCs ().

Figure 3

Co-culture with USCs inhibited the NK cytotoxicity. USC-TA+, USC-TA−, BMSCs, and SMCs (target cells, 1×105 cells/mL; 50 µL/well) were co-cultured with NK-92MI cells (effectors) at E:T ratios of 20:1, 10:1, 5:1, and 1:1 for 4 h. The target cells lysis was determined by measuring the absorbance at 490 nm, as described in Methods. *, P<0.05, post-hoc paired-comparisons. BMSC, human bone marrow mesenchymal stem cells; SMC, human smooth muscle cells; USC TA+, human urine derived stem cells with high telomerase activity; USC TA−, human urine derived stem cells with low telomerase activity; NK, human natural killer cells.

USCs exhibited a specific cytokine release profile

Finally, the cytokines and chemokines released by USCs to the supernatants when cultured in absence of PBMNCs and in direct or indirect contact with PBMNCs were evaluated (). After PBMNCs stimulation, the levels of two immunoregulatory cytokines, IL-6, IL-8, and one chemokine MCP-1 (monocyte chemotactic protein-1) were significantly up-regulated in BMSCs, USC-TA+, and USC-TA− (all P<0.05). In addition, the direct contact mixed culture with PBMNCs induced a higher release of IL-8 and MCP-1 by USC-TA+ and USC-TA−, when compared to that obtained from the same cells culturing supernatant of indirect mixed cultures with PBMNCs in hanging transwell insert. The expression of other cytokines, including RANTES (regulated upon activation, normal T cell expressed and presumably secreted), GROα (growth-regulated oncogene α), and GM-CSF (granulocyte-macrophage colony stimulating factor) was also up-regulated in BMSCs, USC-TA+, and USC-TA− upon PBMNCs stimulation, especially with direct contact mix culture ().

Figure 4

USC showed a characteristic cytokine release profile. The supernatants from USC-TA+, USC-TA−, and BMSCs cultured alone or co-cultured with PBMNCs (direct mixed culture with PBMNCs, or indirect mixed culture with PBMNCs in transwell insert for 48 h) (A) were assessed for their relative levels of cytokines and chemokines by using the human cytokine array panel A, as described in “Methods” (B). A: human cytokine array panel template; B: PBMNCs background; C: USC-TA+ culture alone; D: USC-TA− culture alone; E: BMSCs culture alone; F: USC-TA+ direct mix culture with PBMNCs; G: USC-TA− direct mix culture with PBMNCs; H: BMSCs direct mix culture with PBMNCs; I: USC-TA+ in-direct mix culture with PBMNCs in transwell insert; J: USC-TA− in-direct mix culture with PBMNCs in transwell insert; K: BMSCs in-direct mix culture with PBMNCs in transwell insert: The immunoblot of cytokine expression levels were visualized and quantifed (C). *, P<0.05, comparing with BMSCs alone; †, P<0.05, comparing direct and indirect mixed culture with PBMNCs. BMSC, human bone marrow mesenchymal stem cells; SMC, human smooth muscle cells; USC TA+, human urine derived stem cells with high telomerase activity; USC TA−, human urine derived stem cells with low telomerase activity; PBMNC, human peripheral blood mononuclear cells.

Discussion

This study demonstrated that human USCs express immunological markers and possess immunomodulatory properties in similar levels to MSCs. USCs significantly inhibited the proliferation of PBMNCs in a co-culture system and inhibited the cytotoxicity activity of NK cells. Furthermore, USCs significantly increased the secretion of immunoregulatory cytokines such as IL-6, IL-8 and the immunoregulatory chemokine MCP-1 when the cells were contacting with PBMNCs.

From the histological point of view, USCs constitute a renal parietal cell linage and are different from MSCs; however, USCs appear to have similar characteristics to MSCs. The flow cytometry data showed that almost the whole isolated USCs population homogenously expressed embryonic/mesenchymal stem cell markers, but not hematopoietic and B cell markers, suggesting that isolated USCs possessed the MSCs potency. This surface expression pattern agreed with the ones described in previous studies of USCs (16,19,20). Otherwise, CD80 and CD86 are co-stimulatory molecules located on the antigen presenting cells which mediate T-cell inhibitory signals by interacting with CD152 on activated T cells (21). Our results showed both BMSCs and USCs tested negative for the presence of CD80 and CD86. Regarding immunological markers, USCs contained HLA-ABC antigens (major histocompatibility complex class I, MHC-I), while lacked the expression of HLA-DR (MHC-II) and HLA-G (MHC-I), similarly to BMSCs (22). HLA-DR mismatch is an important factor leading to graft loss after transplantation (23). The absence of co-stimulatory molecules and MHC-II markers on cultured USCs suggested that they possessed hypoimmunogenic properties, allowing them to escape their recognition by the recipient’s immune system. Taken together, these data suggested that the isolated USCs expressed immunomodulatory surface markers, highly resembling to those of MSCs. USCs shared similar stem cell markers with BMSCs, but also expressed different ones, suggesting that USCs might be a new type of adult stem cells with hypoimmunogenic characteristics that require further characterization.

MSCs, even from different origins, possess significant immunomodulatory potential. Since USCs may be an optimal source for stem cell therapy in cases of immune dysfunction (4), we evaluated their immunomodulatory potential. PBMNCs proliferate when co-cultured with other cells due to alloantigen stimulation (24). In this study, USCs were capable of down-regulation alloantigen-driven proliferation of PBMNCs both in one-way and two-way MLR cultures, exhibiting a comparable immunomodulatory potential to that of BMSCs. Our findings are in line with previous studies (19,20). Due to the hypoimmunogenic property, MSCs can escape from the recognition by T cells (25), cytotoxic T lymphocytes (26), NK-T cells (27), and NK cell-mediated lysis (28). In this study, the NK cytotoxicity assay showed that both USC-TA+ and USC-TA− induced less NK cytotoxicity than SMCs at various E:T ratios, and the difference between USC-TA+ and BMSCs at the E:T ratio 10:1 was significant (P=0.013). Taken together, these results suggested that USCs possessed a comparable or even better immunomodulatory property than that of BMSCs.

MSCs have immunomodulatory functions which are exerted by direct cell-to-cell contacts, secretion of cytokines and/or by a combination of both mechanisms, effects of MSCs immunosuppressive are determined by the local conditions of the microenvironment, pro-inflammatory cytokines and chemokines may induce secretion of anti-inflammatory immunosuppressive factors (29). In this study, human cytokine release arrays showed that the levels of immunoregulatory cytokines, IL-6, IL-8, and immunoregulatory chemokine MCP-1 were significantly elevated after USC-TA+ and USC-TA− stimulation with PBMNCs. In addition, the direct contacting of USCs with PBMNCs induced a higher release of IL-8 and MCP-1 than that detected in indirect contacting culture with PBMNCs in hanging transwell insert. The elevated levels of IL-8 and MCP-1 in USCs (both TA+ and TA−) were significantly higher than those in BMSCs, especially mix-culture directly contact with PBMNCs. The concentration of other cytokines, including RANTES, GROα, and GM-CSF were also up-regulated upon PBMNCs stimulation. These cytokines might play a role in the mechanisms underlying the USC-induced inhibition of immune cells proliferation as well as cytotoxicity effects, reveal the immunomodulatory properties of USCs, which grants further investigation.

Due to the high telomerase activity, USCs possess a highly proliferative potential that can generate a large number of cells from a single clone (17). Qin et al. previously showed that USCs with high telomerase activity can be maintained for up to 20 passages, while USCs with low telomerase activity can grow for only 8 to 10 passages (30). To address the effect of telomerase activity on the immunomodulatory properties of USCs, USC-TA+ and USC-TA− clones from the same donor were isolated and expanded. In the current study, the MLR and NK cytotoxicity assays indicated the absence of a significant difference between the inhibitory effects of USCs-TA+ and USCs-TA−, suggesting that the telomerase activity seemed to have little or no effect on the immunomodulatory properties of USCs, even though the USC-TA+ cells were more easily expanded to a suitable quantity for clinical usage. However, it is worth to further address in vivo whether USC-TA+ can maintain their immunomodulatory properties for longer periods than USC-TA− cells.

Several limitations exist in the current study that need to be addressed in the future. Although correlation between the USCs telomerase activity and their immunomodulatory properties was not significant in this study, it is still worth to further investigate whether the telomerase activity influences the immunomodulatory properties of USCs depending on the cell passage number or donor age. In addition, even though we observed that the PBMNCs stimulation enhanced the USCs secretion of immunoregulatory cytokines and chemokines, especially IL-6, IL-8, and MCP-1, the correlation between elevated cytokine levels and USCs immunomodulatory properties and the underlying mechanism remain to be investigated. Furthermore, the immunomodulatory capacity of USCs needs to be evaluated in an in vivo model. All these concerns will be addressed in the following study.

Conclusions

This study we investigated the USCs immunomodulatory effects. Our results showed that USCs expressed typical MSC-like surface cell markers and possessed good immunomodulatory properties, comparable to those of BMSCs. Moreover, interacting with PBMNCs increased the secretion of immunoregulatory cytokines by USCs, especially with direct contacting with immune cells. Therefore, our findings provided a better understanding of the USCs immunomodulatory capacities for their potential application in tissue repair and cell therapy.

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