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Introduction

Pulmonary hypertension (PH) is a type of lung disease that is severely detrimental to human health, and is often characterized by a progressive increase in pulmonary arterial pressure, eventually resulting in right ventricular overload and finally, heart failure (1). Despite current treatments, including the use of targeted medicine such as sildenafil, assisting in relief of the clinical symptoms of PH, the long-term prognosis remains poor (2). For example, the 5-year survival rate of cystic fibrosis patients with PH is 40.8% (3); however, even following lung transplantation, the median survival rate is only ~7 years (4). Therefore, there is an urgent requirement for the development of more effective therapeutic agents for the treatment of PH.

Numerous studies have served to elucidate the mechanism of PH, highlighting the importance of inflammation and the calcineurin (CaN)/nuclear factor of activated T cells (NFAT) signaling pathway (5–13). It has been determined in experimental animal models and in human patients that inflammatory cells are present in the region of remodeled pulmonary arteries (5–8). Furthermore, it has been explicated that the perivascular accumulation of inflammatory cells is essential to pulmonary vascular remodeling (9). Therefore, elevated production of inflammatory cytokines has the potential to be utilized as a predictive marker of survival in patients with PH (9). It remains uncertain as to whether inflammation initiates pulmonary vascular remodeling, or whether it is a bystander effect. However, it is clear that inflammation and associated inflammatory cytokines are involved in the progression of PH. Of the various inflammatory cytokines, the role of tumor necrosis factor-α (TNF-α) in the overproliferation of pulmonary artery smooth muscle cells (PASMCs) and in vascular remodeling, appears to be significant. TNF-α has the ability to cause calcium influx and promote the proliferation of SMCs (10); the activation of the CaN/NFAT signaling pathway is a crucial step within this process (11–13). Therefore, we hypothesize that inflammation-associated overproliferation of PASMCs is a therapeutic target in the treatment of PH.

Mesenchymal stem cells (MSCs), as primitive cells capable of multilineage differentiation and self-renewal, have been observed to effectively inhibit the production of inflammatory cytokines (14), and improve hypoxia-induced PH in experimental animal models (15). However, there are a number ethical factors that may serve to impede the progress of MSCs into the clinic. Our previous study indicated that the immunosuppressive effect of MSCs are strongly associated with their ability to express immuno-regulatory cytokines and secrete prostaglandin E2 (PGE2) (14). It was also revealed that conditioned media from MSCs could produce cytoprotective effects (15). However, the mechanism by which MSC-conditioned media (CM) suppresses the inflammation-associated overproliferation of PASMCs remains unknown.

In the present study, a rat model of PH and a co-culture system comprised of PASMCs and activated T cells were used to assess the ability of MSC-CM to suppress the overproliferation of PASMCs. Associated factors, including the expression levels of TNF-α in the rat model and co-culture system, and the expression levels and activation of CaN/NFAT in PASMCs, were also evaluated, in order to better understand the mechanism by which MSC-CM leads to the overproliferation of PASMCs in PH.

Materials and methods

Preparation of MSC-CM

All studies were approved by the Institutional Review Board of Guiyang Medical College (Guiyang, China) and written informed consent was obtained from all donors. In June 2013, 3 umbilical cords were obtained following normal deliveries from healthy, post-partum women (age, 26–30 years; gestational age, 37–42 weeks) at the Tianjin Central Hospital of Gynecology and Obstetrics (Nankai, China). From these, human umbilical cord-derived MSCs were isolated and cultured in Dulbecco's modified Eagle's medium (DMEM)/F-12 medium (Gibco; Thermo Fisher Scientific, Inc., Waltham, MA, USA) supplemented with 10% fetal bovine serum (FBS; GE Healthcare Life Sciences, Logan, UT, USA) and Gibco penicillin-streptomycin (100 U/ml; Thermo Fisher Scientific, Inc.), as described in a previous protocol (16). MSCs were identified by analyzing the expression of cell-surface markers or internal cell markers was assessed using a BD FACSCalibur flow cytometer (BD Biosciences, Franklin Lakes, NJ, USA), including cluster of differentiation (CD)11b, CD29, CD34, CD44, CD45, CD54, CD73, CD80, CD86, CD90, CD105, human leukocyte antigen (HLA)-DR, HLA-ABC, Nestin and SRY box-2 (Sox-2). The osteogenic and adipogenic differentiation in vitro were also assessed (16). Briefly, MSCs were seeded in 24-well plates at a density of 104 cells/ml (1 ml/well); after 24 h of culture, the medium was replaced with osteogenic or adipogenic induction medium. For osteogenic induction, this medium consisted of DMEM/F-12 medium supplemented with 10% FBS, 100 nmol/l dexamethasone, 10 mmol/l β-glycerophosphate and 0.2 mmol/l L-ascorbic acid-2-phosphate (all Sigma-Aldrich, St. Louis, MO, USA). For adipogenic induction, the medium consisted of DMEM/F-12 medium supplemented with 10% FBS, 5 g/ml insulin, 1 mmol/l dexamethasone, 60 mmol/l indomethacin, and 0.5 mmol/l isobutylmethylxanthine (all Sigma-Aldrich). After 2 weeks of inducted culture, osteogenic and adipogenic differentiation were identified using Alizarin Red S and Oil Red O stain (Sigma-Aldrich), respectively. MSCs passaged 8–10 times were washed thoroughly with phosphate-buffered saline (PBS; BD Biosciences) and incubated in new medium for 24 h. The MSC-CM was collected by centrifugation at 4°C, at 2,000 × g for 10 min, then stored at −80°C. For administration to rats, MSC-CM prepared according to the aforementioned protocol was replaced with serum-free TheraPEAK MSCGM-CD medium (Lonza Group Ltd., Basel, Switzerland) at passage 3.

Experimental animals

All animal studies were approved by the Institutional Animal Care and Use Committee of Guiyang Medical College. Female Sprague-Dawley (SD) rats (age, 8–10 weeks; n=18) with body weights of ~200 g were purchased from and housed in specific pathogen-free units of the Laboratory Animals Center at Tianjin Blood Diseases Hospital (Tianjin, China). The rats were maintained at ~25°C, a relative humidity of 70% and with a 12-h light/dark cycle.

The rats were randomly divided into three equal groups (n=6 per group), as follows: A PH model group, a MSC-CM administration group and a control group. The PH model was induced by a single subcutaneous injection with monocrotaline (MCT; 60 mg/kg; Sigma-Aldrich), in accordance with a previous study (17). On days 5–9 after injection with MCT, 500 µl serum-free MSCGM-CD was subcutaneously injected into the MSC-CM group. The control group was injected with 500 µl PBS alone. Rats were anesthetized by intraperitoneal injection of pentobarbital (50 mg/kg; Sigma-Aldrich) 21 days after administration, and right ventricular systolic pressure (RVSP) and mean aortic pressure (MAoP) were determined, according the protocol detailed in a previous study (18).

Subsequent to the aforementioned procedures, rats were sacrificed by decapitation, lung tissues were removed and fixed in 10% paraformaldehyde at room temperature for 24 h. Serial sections (5 µm) were stained with hematoxylin and eosin (Yuanmu Biotechnology Co., Ltd., Shanghai, China), and the medial wall thickness (WT) of pulmonary arterioles was observed under an Olympus BX53 microscope (Olympus Corporation, Tokyo, Japan) and expressed as: WT (%) = [(medial thickness × 2) / external diameter] × 100 (19).

Immunohistochemical staining for TNF-α in lung tissue

Serial sections (5 µm) were fixed on gelatin-coated slides. Following deparaffinization with two changes of xylene, rehydration with graded ethanol and sequential incubation for 5 min at room temperature with 0.3% Triton X-100 (Sigma-Aldrich) and 3% hydrogen peroxide (Santa Cruz Biotechnology, Inc., Dallas, TX, USA), the sections were incubated with goat polyclonal primary antibody against TNF-α (1:400 dilution; cat. no. sc-1350; Santa Cruz Biotechnology, Inc.) for 12 h at 4°C. Following three washes with PBS, the sections were incubated for 30 min at room temperature with biotinylated rabbit anti-goat monoclonal antibody (1:100 dilution; cat. no. BA-1006; Wuhan Boster Biological Technology, Ltd., Wuhan, China), and the immunoreactivity detected with a 3-amino-9-ethylcarbazole peroxidase substrate kit (Wuhan Boster Biological Technology, Ltd.). The sections were counterstained with hematoxylin, and observed under the Olympus BX53 microscope. Mean optical density (OD) was subsequently calculated using Image-Pro Plus Software 6.0 (Media Cybernetics, Rockville, MD, USA).

Isolation of PASMCs and T cells

A total of 4 SD rats with body weights of ~100 g were sacrificed by decapitation prior to harvesting of pulmonary arteries for PASMC culture using the tissue explants method (20). DMEM/F-12 media supplemented with 10% FBS and 100 U/ml penicillin-streptomycin was used. PASMCs were identified by immunofluorescent staining for α-smooth muscle actin as follows: PASMCs were sequentially fixed with 4% paraformaldehyde for 15 min, incubated with 0.3% Triton X-100 and 1% bovine serum albumin for 20 min at room temperature and incubated with rabbit α-smooth muscle actin polyclonal antibody (α-SMA; 1:100 dilution; cat. no. 14395-1-AP; ProteinTech Group, Inc., Chicago, IL, USA) overnight at 4°C. Subsequent to washing with PBS, cells were incubated with fluorescein isothiocyanate-conjugated goat anti-rabbit immunoglobulin G (1:100 dilution; cat. no. SA00003-2; ProteinTech Group, Inc.) for 2 h at room temperature in the dark. Finally, cells were incubated with DAPI (1 µg/ml) for 5 sec. To extract T cells, the spleens were harvested and T cells were isolated contingent on their non-adherence to nylon wool (21) and stored at −80°C prior to use.

Co-culture of PASMCs and T cells

The cells were divided into three groups, as follows: Group A (PASMCs alone), Group B (PASMCs + T cells) and Group C (PASMCs + T cells + MSC-CM). All cells were maintained at 37°C in a humidified environment with 5% CO2. PASMCs at passage 5 were seeded into 24-well plates at a density of 104 cells/ml (1 ml/well). In Group A, the media was renewed after 24 h of culture. In Group B, 0.9 ml of medium was removed, and 0.9 ml T cell suspension at a density of 105 cells/ml was added and stimulated by concanavalin A (ConA; 10 µg/ml; Sigma-Aldrich). For Group C, the total volume of supernatant was removed and ConA-stimulated T cells were added at the same density as those in Group B. Furthermore, an additional 0.1 ml MSC-CM was added.

TNF-α protein expression levels in co-culture systems

Following 3 days of co-culture, the cell-free supernatant was collected from each cell group by centrifugation (4°C, 2,000 × g, 10 min), and expression levels of TNF-α were measured using a Rat TNF-α Mini ABTS ELISA Development kit (PeproTech, Inc., Rocky Hill, NJ, USA), according to the manufacturer's protocol.

Proliferation of PASMCs

Following collection of the supernatant from all three groups, T cells were removed by washing three times with PBS. Next, PASMCs were incubated for 4 h in 300 µl new medium containing 15 µl 3-(4, 5-diethylthiazol-2-yl)-5-(3-carboxymethoxyphenyl)-2-(4-sulfophenyl)-2H-etrazolium, inner salt (MTS; Promega Corporation, Madison, WI, USA) at 37°C/5% CO2. The OD of the supernatant was read at 490 nm using a Model 680 microplate reader (Bio-Rad Laboratories, Inc., Hercules, CA, USA).

mRNA expression of CaN and NFATc2

After 3 days of co-culture, total RNA of PASMCs was extracted from each of the three groups using an E.Z.N.A. Total RNA I kit (Omega Biotek, Inc., Norcross, GA, USA), and reverse transcribed to cDNA using a Moloney Murine Leukemia Virus Reverse Transcriptase kit (Invitrogen; Thermo Fisher Scientific, Inc.). Following this, the cDNA was amplified and the expression of CaN and NFATc2 were analyzed by quantitative PCR (qPCR) using an Applied Biosystems 7300 Real-Time PCR System with Invitrogen Platinum SYBR Green qPCR SuperMix-UDG w/ROX (Thermo Fisher Scientific, Inc.). The PCR cycling conditions were as follows: 95°C for 2 min, 95°C for 15 sec and 60°C for 30 sec; this was repeated for 40 cycles, as per our previous study (22). Relative expression levels were quantified by the 2−ΔΔCq normalization method (23). The primers used are listed in Table I.

Table I. Rat gene primers for RT-qPCR.

Table I.

Rat gene primers for RT-qPCR.

Primer	Sequence
GAPDH F	5′-CCATTCTTCCACCTTTGATGCT-3′
GAPDH R	5′-TGTTGCTGTAGCCATATTCATTGT-3′
CaN F	5′-CAGAGGGTGCTTCGATTCTC-3′
CaN R	5′-CCCCTAAGAAGAGGTAGCGA-3′
NFATc2 F	5′-CAGCAGATTTGGGAGATGGAAG-3′
NFATc2 R	5′-GACTGGGTGGTAAGTAAAGTGC-3′

[i] F, forward; R, reverse; CaN, calcineurin; NFATc2, nuclear factor of activated T cells c2; RT-qPCR, reverse transcription-quantitative polymerase chain reaction.

CaN activity

PASMCs from each of the three groups were lysed in 1 ml lysate buffer composed of 50 mmol/l Tris, 0.5 mmol/l DTT, 50 µg/ml PMSF, 50 µg/ml soybean trypsin inhibitor, 5 µg/ml leupeptin and 5 µg/ml aprotinin (Beijing Dingguo Changsheng Biotechnology Co., Ltd., Beijing, China). Following three freeze-thaw cycles, the supernatant was collected by centrifugation (4°C, 2,000 × g, 10 min) for measurement of CaN phosphatase activity using a Calcineurin assay kit (Nanjing Jiancheng Bioengineering Institute, Nanjing, China).

NFATc2 activation

After 3 days of co-culture, PASMCs from each of the three groups were sequentially fixed with 4% paraformaldehyde (15 min), incubated with 0.3% Triton X-100 and 1% bovine serum albumin (20 min), and then incubated with mouse anti-rat NFATc2 monoclonal antibody (1:100 dilution; cat. no. NB300-504; Novus Biologicals, LLC, Littleton, CO, USA) overnight at 4°C. Subsequent to washing with PBS, cells were incubated with fluorescein isothiocyanate-conjugated goat anti-mouse immunoglobulin G (1:100 dilution; cat. no. SA00003-1; ProteinTech Group, Inc.) for 2 h at room temperature in the dark. Finally, cells were incubated with DAPI (1 µg/ml) for 5 sec and assessed with a TCS SP5 confocal laser scanning microscope (Leica Microsystems GmbH, Wetzlar, Germany).

Statistical analysis

Data are presented as mean ± standard deviation and SPSS software (version 17.0; SPSS, Inc., Chicago, IL, USA) was used for statistical analysis. Differences were compared using an independent-samples t-test or one-way analysis of variance. P<0.05 was considered to indicate a statistically significant difference.

Results

Identification of MSCs and PASMCs

Human MSCs grown in the serum-free medium presented with a typical fibroblastic shape (Fig. 1A), whilst those cultured in the specific conditioned medium displayed osteogenic (Fig. 1B) and adipogenic (Fig. 1C) differentiation. The MSCs were positive for HLA-ABC (99.73%), Nestin (68.39%), Sox-2 (78.46%), CD29 (100%), CD44 (100%), CD54 (86.98%), CD73 (99.79%), CD90 (100%) and CD105 (97.33%), and negative for CD34, CD45, CD80, CD86, HLA-DR and CD11b (Fig. 1D).

Figure 1. Growth of mesenchymal stem cells (MSCs) and pulmonary artery smooth muscle cells (PASMCs) in vitro. (A) MSCs culured in serum-free medium at passage 3 (magnification, ×100). (B) Osteogenic and (C) adipogenic differentiation of MSCs cultured in MSC-conditioned media identified using Alizarin red S or Oil Red O stain, respectively (magnification, ×200). (D) Phenotypic analysis of MSCs, assessed using flow cytometry. (E) PASMC tissue explant cultured for 5 days (magnification, ×100). (F) PASMCs at passage 3 (magnification, ×100). (G) PASMC immunofluorescent staining for α-smooth muscle actin (magnification, ×200). CD, cluster of differentiation; Sox-2, SRY box-2; HLA, human leukocyte antigen.

After 5 days of culture using the tissue explants method, PASMCs harvested from rats were observed surrounding the tissue explants (Fig. 1E). Following a further 3 passages of culture, the cells displayed the typical ‘hill and valley’ growth pattern (Fig. 1F), and were positive for α-SMA, according to immunofluorescent staining (Fig. 1G).

MSC-CM improves PH

The examination of hemodynamics 21 days after injection of MCT indicated a significant increase in RVSP compared with the control group (48.26±3.93 vs. 27.58±3.47 mmHg; P<0.01; Fig. 2A), and a significant decrease in MAoP compared with the control group (89.54±15.81 vs. 116.37±16.17 mmHg; P<0.05; Fig. 2B). In accordance with this finding, histological examination also indicated that, 21 days after injection with MCT, medial hypertrophy of pulmonary muscular arterioles was evident in the model group (Fig. 2B). Additionally, WT levels were significantly increased in the model group compared with the control (34.12±3.59 vs. 12.53±1.82%; P<0.01; Fig. 2C). These changes indicated the development of PH in the experimental rat.

Figure 2. Effects of MSC-CM on monocrotaline-induced pulmonary hypertension. Left panels: Histological examination of lung tissue in (A) control, (B) model and (C) MSC-CM treatment groups (hematoxylin and eosin stain; magnification, ×400). Right panels: Changes of (A) RVSP, (B) MAoP and (C) medial WT in each group. Data are presented as mean ± standard deviation (n=6). *P<0.01, **P<0.05. RVSP, right ventricle systolic pressure; MSC-CM, mesenchymal stem cell-conditioned media; MAoP, mean aortic pressure; WT, wall thickness.

Administration of MSC-CM leads to the improvement of abnormal hemodynamics

RVSP decreased to 31.42±3.38 mmHg (Fig. 2A) and MAoP increased to 112.97±14.26 mmHg (Fig. 2B) following MSC-CM treatment; these values were significantly different compared with the model group (P<0.05). In addition, the medial hypertrophy of pulmonary muscular arterioles was improved (Fig. 2C), and the WT was significantly decreased (13.28±1.78%) compared with that in the model group (34.12±3.59%; P<0.01; Fig. 2C).

MSC-CM decreases the protein expression levels of TNF-α in lung tissue

Compared with the control group (Fig. 3A), immunohistochemical staining revealed that an abundance of cells were positive for TNF-α within the lung tissue 21 days after injection of MCT in the model group (Fig. 3B). Following the administration of MSC-CM, the number of cells positive for TNF-α decreased (Fig. 3C), and the average OD significantly decreased from 0.23±0.07 in the model group to 0.17±0.06 in the MSC-CM treatment group (P<0.01; Fig. 3D).

Figure 3. Protein expression levels of TNF-α in lung tissue. Immunohistochemical staining for TNF-α in the (A) control, (B) model and (C) MSC-CM treatment groups (3-amino-9-ethylcarbazole peroxidase staining; magnification, ×400). (D) Quantified expression levels of TNF-α in lung tissue. Data are presented as mean ± standard deviation (n=6). *P<0.01. TNF-α, tumor necrosis factor-α; MSC-CM, mesenchymal stem cell-conditioned media; AOD, average optical density.

MSC-CM suppresses the production of TNF-α and proliferation of PASMCs in co-culture systems

After 3 days of culture, levels of TNF-α in the supernatant of the co-culture system were analyzed by ELISA. The results revealed that high levels of TNF-α (762.51±42.35 pg/ml) were produced by T cells under stimulation with ConA (Fig. 1A). However, in the presence of MSC-CM, the production of TNF-α was significantly inhibited (218.25±19.33 pg/ml; P<0.01; Fig. 4A). Additionally, the proliferation of PASMCs, as assessed by an MTS assay, revealed that the proliferation of PASMCs significantly increased when co-cultured with ConA-stimulated T cells, compared with PASMCs cultured alone (0.94±0.05 vs. 0.73±0.06; P<0.01; Fig. 4B). Furthermore, the ability of T cells in promoting the proliferation of PASMCs was significantly inhibited by treatment with MSC-CM (0.78±0.07; P<0.01; Fig. 4B).

Figure 4. Changes in TNF-α, CaN and NFATc2 in the co-culture system. (A) Protein expression levels of TNF-α in the supernatant. (B) Proliferation of PASMCs. mRNA expression of (C) CaN and (D) NFATc2 in PASMCs. (E) CaN activity in PASMCs. Group A, PASMCs alone; Group B, PASMCs + T cells; Group C, PASMCs +T cells + MSC-CM. Data are presented as mean ± standard deviation (n=6). *P<0.01. Activation of NFATc2 in PASMCs in the co-culture system for (F) group A; (G) group B, and (H) group C (fluorescein isothiocyanate/DAPI staining; magnification, ×400). TNF-α, tumor necrosis factor-α; PASMCs, pulmonary artery smooth muscle cells; MSC-CM, mesenchymal stem cell-conditioned media; OD, optical density; CaN, calcineurin; NFATc2, nuclear factor of activated T cells c2.

MSC-CM downregulates the expression of CaN and NFATc2

CaN and NFATc2 are critical regulatory factors of SMC proliferation, thus, the expression levels of both were assessed by reverse transcription-quantitative polymerase chain reaction (11). The results indicated that, after 3 days of co-culture with ConA-stimulated T cells, the expression levels of CaN and NFATc2 in PASMCs were significantly upregulated compared with the expression in PASMCs alone. Furthermore, MSC-CM was able to significantly reduce the expression levels of CaN and NFATc2 (P<0.01) that were increased by the promoting effects of the activated T cells (Fig. 4C and D).

MSC-CM suppresses CaN activity and NFATc2 activation in PASMCs

In the co-culture system, it was observed that intracellular CaN activity was significantly upregulated in PASMCs cultured for 3 days with ConA-stimulated T cells, compared with PASMCs cultured alone (0.59±0.06 vs. 0.32±0.04 U/mgprot; P<0.01; Fig. 4E). Furthermore, the majority of NFATc2 was translocated to the nucleus, indicating the activation of NFATc2 (Fig. 4G). Following the addition of MSC-CM, the intracellular CaN activity of PASMCs was significantly decreased (0.37±0.06 U/mgprot; P<0.01; Fig. 4E). When PASMCs were cultured independently, the expression of NFATc2 was predominantly localized to the cytoplasm (Fig. 4F). Finally, addition of MSC-CM also led to suppression of NFATc2 activation (Fig. 4H).

Discussion

The present study demonstrated that the administration of MSC-CM decreases protein expression levels of TNF-α in the lungs of rat models with MCT-induced PH. In addition, improvements in hemodynamic and histological abnormalities were also observed. A co-culture system comprised of activated T cells and PASMCs was established to further reveal the therapeutic mechanism of MSC-CM in PH. The in vitro co-culture system revealed that the high levels of TNF-α produced as a result of activated T cells leads to the upregulation of CaN and NFATc2 expression. Additional effects observed included an increase in intracellular CaN activity and NFATc2 activation in PASMCs, thus promoting the proliferation of PASMCs. MSC-CM was able to effectively suppress the production of high levels of TNF-α by T cells, which led to the downregulation of expression levels of CaN and NFATc2 in PASMCs. This had the effect of decreasing CaN activity and preventing NFATc2 activation, which consequently resulted in suppression of the proliferation of PASMCs.

Persistent contraction and hypertrophy of pulmonary arterioles are considered to be defining characteristics of PH (24). Inflammation and the overproliferation of PASMCs are also hypothesized to have an involvement in the pathological process, thus rendering them a therapeutic target for the treatment of PH (12). MSCs, as a subset of stromal stem cells, have attracted much attention as potential therapeutic vehicles for the treatment of PH and other diseases of the lung, due to their potent immunomodulatory, anti-inflammatory and anti-fibrotic properties (25–27). Previously, it has been demonstrated that MSCs have the ability to suppress activated CD4+ T cells, thereby preventing the production of inflammatory cytokines when co-cultured (14). Furthermore, the immunosuppressive activity of MSCs is highly associated with the secretion of PGE2 and immunoregulatory cytokines (14). Due to the extensive level of inflammation involved in the pathological mechanism of PH, the immunosuppressive effects of MSCs may be beneficial to the treatment of PH. The exact mechanism detailing the involvement of MSCs in PH, however, remains unclear. A former hypothesis suggesting that MSCs had the ability to differentiate into various lung tissue types following transplantation has been somewhat discredited due to the existence of the MSC niche, which may serve to hinder the homing and differentiation of MSCs (28). Furthermore, due to the ability of MSC-CM to attenuate hypoxia-induced pulmonary injury (15), the paracrine mechanism is generally considered to have greater plausibility in explaining the protective effects of MSCs. With the additional benefit of no ethical restrictions against its use, MSC-CM, which possesses numerous therapeutic effects, may be a promising vehicle in the clinic. In the present study, a rat model of MCT-induced PH was used to assess the immunoregulatory capabilities and therapeutic effects of MSC-CM. The results demonstrated that expression levels of TNF-α within the lung tissue were decreased by the immunosuppressive activity of MSC-CM. As a result, hemodynamic abnormalities, including increased RVSP and decreased MAoP, were improved and approaching normal levels. Further examination of the hemodynamics also indicated that the medial hypertrophy and remodeling of pulmonary arterioles were prevented. These results may indicate the mechanisms by which the immunoregulatory properties of MSC-CM are responsible for potential therapeutic benefits in the treatment of PH.

The NFAT family of proteins contains a series of pivotal regulators of immune response that are widely expressed in a host of tissues and organs (29), including smooth muscle cells (30). Typically, NFAT proteins are predominately distributed in the cytoplasm, where they are inactive. Upon dephosphorylation by the Ca2+-responsive phosphatase CaN, NFAT proteins are activated and translocated to the nucleus in order to exert their regulatory actions (29). It has previously been identified that the activation of CaN and NFAT are involved in the pathogenesis of PH (9).

NFAT activation has been observed in PASCs obtained from patients with PH (12) and in experimental animal models, such as MCT-induced (12) and hypoxia-induced (13) PH models. Furthermore, inhibition of CaN or NFAT may result in a decrease in the proliferation of PASMCs, and an increase the levels of apoptosis (12), thereby inhibiting hypoxia-induced PH and right ventricular hypertrophy (31). In order to further elucidate the exact therapeutic mechanism of MSC-CM in PH, the present study used an in vitro co-culture system containing T cells and PASMCs. The supernatant protein expression levels of TNF-α, mRNA expression levels of CaN and NFAT, as well as CaN activity and NFATc2 activation in PASMCs were assessed to better understand the mechanisms pertaining to the regulatory effects of MSC-CM on the inflammation-associated overproliferation of PASMCs. The results indicated that, under the stimulation of ConA, T cells produced high levels of TNF-α, resulting in the upregulation of CaN and NFAT mRNA expression levels, increased CaN activity, and promoted activation of NFATc2, thus accelerating the proliferation of PASMCs. As a result of the immunosuppressive effects of MSC-CM, TNF-α production levels significantly decreased. This immunosuppressive effect was also associated with downregulated expression levels of CaN and NFAT in PASMCs; in agreement, CaN activity and NFATc2 activation levels were observed to have decreased. Consequentially, the overproliferation of PASMCs was effectively suppressed by MSC-CM.

In conclusion, the present study provides new evidence highlighting the ability of conditioned media from MSCs to suppress the overproliferation of PASMCs, and thus have possible therapeutic benefits in the treatment of PH. The predominant reason for this effect was a result of the suppression of TNF-α, and the subsequent inhibitory action on the expression levels of CaN and NFAT, CaN activity, and the activation of NFATc2 in PASMCs. However, the long-term impacts and potential side-effects of this prospective treatment require further investigation.

Acknowledgements

The present study was supported by the National Natural Science Foundation of China (grant nos. 30560159, 30960412 and 31360285).

References