Human amnion-derived mesenchymal stem cells protect against UVA irradiation-induced human dermal fibroblast senescence, in vitro

Introduction

Skin is an essential natural barrier protecting body from physical, chemical and microbial hazards, also a visual indicator of body's aging process (1). 90%of the ultraviolet (UV) reaching surface of the earth is long-wavelength irradiation (UVA, 320–400 nm), which can penetrate the epidermis into the dermis. So it is well established that UVA is responsible for skin photoaging induced by UV. Studies demonstrated UVA radiation can induce cytokine expression in human epidermoid carcinoma cells. UVA radiation caused an increased proportion of β-Gal positive cells and reduced telomere length in human skin fibroblasts. In addition, UVA radiation inhibited TGF-β 1 secretion, induced G1 phase arrest, reduced SOD and GSH-Px levels, increased MDA levels and the expression of MMP-1, TIMP-1, p66, p53 mRNA expression (2,3).

Human amnion-derived mesenchymal stem cells (HAMSCs) obtained from human amniotic membrane (AM) are readily available and high abundant tissue, with substantial benefits as seed cells (3,4). Their low anti-flammatory properties and fewer ethical concerns compared with other sources of stem cell are clear advantage (5–7). It is proved that HAMSCs secrete a variety of cytokines, which is essential to a series of basic biological processes of cells (8). Recent studies revealed that HAMSCs have important roles in cell differentiation (9–12), promoting cell proliferation (13–15), enhancing cell viability and function (16–18), protecting cells from adverse effects and inhibiting apoptosis (19,20) in vivo or in vitro. The present study aimed to determine whether HAMSCs involved in the protection of human dermal fibroblasts (HDFs) from UVA-induced senescence.

In order to investigate the protective mechanisms of HAMSCs against UVA-induced HDFs senescence, an in vitro cell-senescence model was built through the exposure of pre-HAMSCs-treated HDFs to UVA, and the effects of HAMSCs on ROS contents and mitochondrial membrane potential (Δψm), HDFs senescence marker genes p53 and MMP1 (21) expression were detected by reverse transcription quantitative polymerase chain reaction analysis and western blot. Furthermore, senescence-associated β-galactosidase (SA-β-Gal) staining was performed to evaluate the senescence status of HDFs. SA-β-Gal activity distinguishes senescent cells from those terminally differentiated, therefore act as a senescence biomarker. Our results showed that HAMSCs up-regulated MERK1/2 in UVA induced senescence HDFs, which means skin senescence might related to ERK1/2 MAPK signal pathway.

Materials and methods

Chemicals and reagents

Fetal bovine serum (FBS), α-minimum essential medium (αMEM), trypsin-EDTA, phosphate-buffered saline (PBS) and penicillin G-streptomycin sulfate were purchased from Gibco Life Technologies (Carlsbad, CA, USA). 2,7-dichlorodihydro fluoresceindiacetate (DCFH-DA) fom Sigma-Aldrich (St. Louis, MO, USA). Transwells (6-well millicell Hanging Cell Culture Inserts, 0.4 µm, PET) and 6-well culture plates were purchased from Millipore Corp. (Billerica, MA, USA). The goat anti rabbit IgG, phosphor-p44/42 MAPK rabbit mAb (p-ERK1/2), JNK MAPK rabbit mAb, p53 rabbit mAb, SIRT1 rabbit mAb and Senescence β-Galactosidase Staining kit were purchased from Cell Signaling Technology, Inc. (3 Trask Lane; Danvers, MA, USA). Penicillin and streptomycin from Gibco Life Technologies. Other reagents used were of the highest commercial grade available.

Cell culture

Human amnion-derived mesenchymal stem cells were prepared as described previously (3). Briefly, human amniotic membrane was mechanically peeled off from the chorion of a placenta obtained from an uncomplicated elective caesarean section with the informed consent of the donor patient. The HAMSCs layer was thoroughly scraped out from the underlying tissues such as the spongy and fibroblast layers. Within 24 h AM layer was then treated with 0.125% trypsin three times each for 20 min to obtain dissociated HAMSCs. The cells were cultured in α-MEM supplemented with 10% FBS, penicillin (100 U/ml) and streptomycin (100 µg/ml), incubated in an incubator at 37°C with 5% CO2 in a humidified atmosphere. The culture medium was changed every 3 days.

Primary HDFs were purchased from Wuxi BioHermes Bio&Medical Technology Co., Ltd. (Wuxi, China). Cultured in a 10-cm dish in α-MEM supplemented with 10% fetal bovine serum, penicillin (100 U/ml) and streptomycin (100 µg/ml).

The Co-culture system

The transwell co-culture system was used to investigate the effects of HAMSCs on HDFs. HDFs were seeded at an initial density of 5×104 cells/cm2 in 6-well culture plates. Transwells were placed in other 6-well culture plates and seed at increasing HAMSCs (5×104 cells/transwell, 10×104 cells/transwell and 15×104 cells/transwell). Immediately after 9 J/cm2 UVA on HDFs to create UVA induced senescence, HAMSCs in transwells moved into the appropriate well of 6-well plate to co-culturing with HDFs. HDFs in wells with HAMSCs on transwells served as the treatment groups, while HDFs without transwells were designated as the control group.

UVA irradiation

24 h after HDFs seeded in the six-well plate, HDFs were exposed to 9 J/cm2 (30 min) UVA irradiation. Cells were washed with phosphate-buffered saline (PBS) and covered with a thin layer of PBS prior to UVA exposure. The culture plate lid was removed, and the 6-well plate was placed on a brass block embedded on ice, in order to reduce any evaporation, at a distance of 15 cm from the UVA light source. As the UVA irradiation source, an Ultraviolet phototherapy instrument (SS-04A; Shanghai Sigma High-tech Co., Ltd., Shanghai, China) equipped with a 15-W ozone-free UVA lamp (CEL015 W; Philips, Groningen, The Netherlands) was used. The incidence dose of UVA was measured with a UVA/UVB-ultraviolet meter (Factory affiliated to Beijing Normal University, Beijing, China). After UVA irradiation, PBS was replaced with culture medium and transwells seeded with HAMSCs were placed in wells of the co-culture group, then they were incubated under standard conditions for 72 h prior to analysis.

Analysis of cellular proliferation

HDFs accepted UVA irradiation then co-cultured with HAMSCs after 72 h, transwells containg HAMSCs were removed and HDFs were harvested. After fixed with 75% ice-cold ethanol at 4°C in the dark, cell cycle fractions (G0, G1, and G2, M phase) were determined by flow cytometry.

SA-β-Gal staining

SA-β-Gal activity was evaluated using a β-galactosidase staining kit (Beyotime Institute of Biotechnology, Haimen, China). Cells were washed with PBS and fixed for 15 min at room temperature with fixative solution. The HDFs cells were then incubated at 37°C overnight. SA-β-Gal-positive staining was expressed as a percentage of the total number of cells; cell numbers were counted in four continuous visual fields using a microscope (Olympus CX51; Olympus, Tokyo, Japan; total magnification, ×20).

Assessment of ROS production

The level of ROS induced by UVA in HDFS was measured using DCFH-DA as a fluorescent probe. After irradiation and co-culturing with HAMSCs, transwells were removed and HDFs were washed three times with PBS, incubated with DCFH-DA (10 mM) for 30 min at 37°C, washed three times with PBS. Macrographs of DCFDA fluorescence were immediately.

Flow cytometry analysis of mitochondrial membrane potential

Mitochondrial membrane potential (Δψm) was analyzed by a fluorescent dye JC-1 (Beyotime Institute of Biotechnology), following manufactur's protocol. JC-1 is capable of selectively entering mitochondria where it forms monomers and emits green fluorescence (530 nm) when Δψm is relatively low. At high Δψm, JC-1 aggregates and gives a red fluorescence (590 nm). Assays were initiated by incubating HDFs with JC-1 for 30 min at 37°C in the dark and the fluorescence of separated cells was detected with a flow cytometer (FAC-SCalibur; BD Biosciences, San Diego, CA, USA). Δψm was determined by a ratio of fluorescence intensity at 590 nm to that at 530 nm. A minimum of 10,000 cells per sample was acquired and analyzed.

Assessment of senescence related RNA and protein

Total RNA was extracted from the cells using TRIzol reagent (Promega Corp., Madison, WI, USA). RNA concentration and purity were determined with a Nanodrop 2000-UV spectrophotometer (Thermo Fisher Scientific, Inc., Waltham, MA, USA). Ribosomal RNA band integrity was evaluated using conventional denaturing agarose gel electrophoresis using the SDS-PAGE gel quick preparation kit (Beyotime Institute of Biotechnology). Equal amounts of RNA (500 ng) from each sample were reverse transcribed using a PrimeScript™ RT Reagent kit with gDNA Eraser (Takara Bio, Dalian, China) according to the manufacturer's instructions. qPCR was performed using SYBR-Green dye method (Premix Ex Taq; Takara Bio) using an ABI700 Real-Time PCR detection system (Applied Biosystems; Life Technologies, Thermo Fisher Scientific, Inc.). The following standard cycling conditions for qPCR were applied: 95°C for 3 min to activate polymerase, 40 cycles of denaturation at 95°C for 15 sec and annealing-extension at 60°C for 30 sec. Melting curve analysis was performed following every run by defined heating up to 95°C to assess the presence of unspecific PCR products. Specific primers for the RT-qPCR reactions were as follows: MMP1 forward, 5′-TTGGAGGGGATGCTCATT-3′ and, reverse, 5′-TAAAACGCAGCTCAGTAACAGTCCG-3′; p53, forward, 5′-AGAATCTCCGCAAGAAAGG-3′, reverse, 5′-GCTGGTATGTCCTACTCCC-3′; β-actin, forward, 5′-TGGAATCTTGCTCTTATTTTCACA-3′ and reverse, 5′-TAAAACGCAGCTCAGTAACAGTCCG-3′. All primers were synthesized by Sangon Biotech, Co., Ltd. (Shanghai, China) and used at 400 nM expect for β-actin at 300 nM. All PCR efficiencies were between 90 and 110%.

At the end of 72 h after UVA irradiation and co-culture, transwells containg HAMSCs were removed and HDFs in each group were lysed in RIPA buffer containg 1 mM phenylmethane sulfonylfuoride according to the manufacturer's instructions. The total protein concentration was determined using a bicinchoninic acid (BCA) assay kit. Protein lysates (20 µg) were separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) and then transferred onto 0.22 µm polyvinylidene difluofide membranes (Millipore Corp.). After blocking, membranes were incubated overnight at 4°C with specific antibodies for the detection of p53 (1:1,000), p38 (1:1,000), SIRT1 (1:1,000), p-ERK1/2 (1:500), ERK1/2 (1:500). After three washes with PBST (0.5% Tween-20 in PBS), the membranes were incubated with the relevant secondary antibodies (1:2,000) for 1 h at 37°C, washed and visualized with an ECL detection kit (Amersham Pharmacia Biotech, Piscataway, NJ, USA). The GAPDH (1:500) served as internal control.

Statistical analysis

Analyses were performed using GraphPad Prism software (GraphPad Inc., La Jolla, CA, USA). Values are presented as the mean ± standard deviation. The one-way analysis of variance was used for comparisons involving more than two groups. P<0.05 was considered to indicate a statistically significant difference.

Results

HAMSCs promoted UVA induced HDFs proliferation and reduce UVA induced HDFs senescence

Flow cytometry were used to measure the proliferation of UVA treated HDFs seeded in the 6-well plates co-culture with HAMSCs. Cell cycle fractions (G0, G1, S, and G2, M phase) were determined by flow cytometry at 72 h after UVA and HAMSCs treatment. The S phase showed significant inhibited treated by UVA, after co-culture with HAMSCs the S-phase checkpoints increased (Fig. 1A). So we chose 10×104 cells/transwell HAMSCs in following experiment. Our results further demonstrated that co-culturing with HAMSCs accelerated UVA-induced HDFs proliferation.

Figure 1. The effect of HAMSCs on UVA induced HDFs proliferation and senescence by flow cytometry and X-gel staining. Transwells containing HAMSCs were moved into the correlating wells containing HDFs which accepted 9 J/cm2 UVA irradiation. (A) HDFs cell cycle fractions (G0, G1, S, and G2, M phase) were detected at 72 h after UVA irradiation and co-culture or without HAMSCs. (B) SA-β-gal staining was taken 72 h after irradiation and co-culturing with/without HAMSCs, the stained surface was measured by image-pro plus 6.0 (IPP) analysis. Values are means ± SD of 3 independent experiments with each performed in triplicate. #P<0.05 vs. the HDFs group; ##P<0.01 vs the HDFs group; *P<0.05 and **P<0.01 compared with the group treated with UVA alone.

X-gal staining results showed that the percentage of cells stained by X-gal following 9 J/cm2 UVA irradiation was markedly increased compared with that of the control group (10.8 and 22.6%, respectively; P<0.05), while HAMSCs attenuated the ratio of positive staining compared with that of the UVA-treated only cells (15.3 and 22.6%, respectively; P<0.05) (Fig. 2B).

Figure 2. Flow cytometry of ROS generation and mitochondria depolarization in UVA irradiated HDFs after co-culturing with or without HAMSCs for 72 h or without. Transwells containing HAMSCs were moved into the correlating wells containing HDFs which just accepted 9 J/cm2 UVA irradiation. (A) Macrogaphs of DCFDA fluorescence was determined by flow cytometry at 72 h after UVA irradiation and co-culturing with/without HAMSCs. (B) JC-1 fluorescence was determined by flow cytometry at 72 h after UVA irradiation and co-culture with or without HAMSCs. ##P<0.01 vs the HDFs group; *P<0.05 and **P<0.01 compared with the group treated with UVA alone. Values are means ± SD of 3 independent experiments with each performed in triplicate.

HAMSCs inhibited ROS generation and mitochondria depolarization in UVA induced HDFs

To elucidate whether the beneficial effects of HAMSCs were linked to their antioxidant properties, the ROS generation in UVA-induced HDFs were measured. Subsequently, the intensity of fluorescence was determined by flow cytometry.

As shown in Fig. 2A, after UVA irradiation, intracellular ROS generation increased significantly. The level of ROS in UVA treated cells was much higher than the level of ROS in control cells throughout the experiment. Co-culture with HAMSCs significantly inhibited the elevated intracellular concentration of ROS.

Loss of mitochondrial membrane potential in cells has been estimated using JC-1 assay kit. In normal cells, JC-1 aggregated in mitochondria and the ratio was 124.29. UVA irradiation treated cells showed the higher ratio 785.22, which indicated the dissipation of Δψm. HDFs treatedwith UVA and co-cultured with HAMSCs demonstrated attenuation of the dissipation of Δψm 288.56 (Fig. 2B). Above results uggested that HAMSCs protect mitochondria depolarization induced by UVA irradiation.

HAMSCs reduced the expression of senescence related markers

Reverse transcription quantitative polymerase chain reaction analysis showed mRNA expression levels of p53 and MMP1 were significantly reduced in UVA-treated HDFs co-cultured with HAMSCs than that of the UVA-treated only group (P<0.05) (Fig. 3A). In order to further study the efficacy of HAMSCs, western blot analysis was to evaluate the protein expression in co-culture with UVA and HAMSCs or with UVA only of HDFs. The result showed that HAMSCs had a significant effect on p53, active-MMP1 and SIRT1 (Fig. 2B).

Figure 3. Expression of senescence related markers. Transwells containing HAMSCs were moved into the correlating wells containing HDFs which accepted 9 J/cm2 UVA irradiation. (A) mRNA expression of MMP1 and p53 in UVA irradiated HDFs co-culturing with or without HAMSCs for 72 h. (B) Expression of p53, MMP1 and SIRT1 in UVA irradiated HDFs co-culturing with or without HAMSCs were determined by western blot, GAPDH served as an internal control. Values are means ± SD of 3 independent experiments with each performed in triplicate. ##P<0.01 vs the HDFs group; **P<0.01 compared with the group treated with UVA alone.

HAMSCs activated ERK1/2 in UVA induced HDFs

EEK1/2 are important members of the MAPK signal pathway, which regulates the differentiation, mineralization and proliferation of HDFs. Fig. 4 showed ERK1/2 in HDFs in respective of UVA treatment after 72 h with or without co-culture with HAMSCs. Higher level of phosohorylated ERK1/2 were observed compared with UVA irradiated HDFs co-cultured with HAMSCs than without. These results suggested that HAMSCs enhance UVA-induced inhibition of ERK1/2, which might play a role in regulating UVA induced HDF senescence.

Figure 4. Expression of ERK1/2, p-ERK1/2 in UVA irradiated HDFs after co-culturing with or without HAMSCs for 72 h. Transwells containing HAMSCs were moved into the correlating wells containing HDFs which accepted 9 J/cm2 UVA irradiation. Densitometric measures of the band intensity are expressed as the signal ratios indicating the level of ERK phosphorylation (p-ERK1/2 ERK1/2). ##P<0.01 vs the HDFs group; **P<0.01 compared with the group treated with UVA alone. Values are means ± SD of 3 independent experiments with each performed in triplicate.

Discussion

HAMSCs has been the shining star in cell-based therapy in recent years, which appear to have several advantages over other stem cell lineages as a cell therapy. Studies showed that HAMSCs can maintain mouse spermatogonial stem cells in an undifferentiated state when cultured long term due to high leukemia inhibitor factor (LIF) expression. HAMSCs had an increased proliferative capacity, higher colony-forming efficiency, fewer apoptotic cells, and similar cell-junction formation capabilities and pump functionality compared with primary HCECs (21,22). Amniotic membrane can restrict dedifferentiation of human retinal pigment epithelial cells (RPE cells) in culture, promoting RPE65, CRALBP, VEGF, CD68, and tyrosinase gene expression in RPE cells (23). Experiments have demonstrated the ability of HAMSCs to migrate into brain, prevents the degeneration of nigral dopmineneurons in rats with 6-hydroxydopami-ne lesions (24). HAMSCs transplantation promotes ovarian function by inhibiting tumor necrosis factor-alpha-mediated cell apoptosis and reducing inflammation in chemotherapy-induced premature ovarian failure (25). HAMSCs are able to produce/release a number of biologically active cytokines/growth modulators, such as basic fibroblast growth factor (bFGF), epithelial growth factor (EGF), insulin growth factor-1 (IGF-1), stem cell factor (SCF), IL-1a, IL-10, insulin, tumor necrosis factor-a, IFN-g, and leukemia inhibitory factor (LIF), some of which could constitute crucial components in maintaining/enhancing the survival/anti-senescence/apoptosis of progenitor/adult cells (26). HAMSCs can secrete several cytokines and growth factors, promoting the survival of the surrounding cells. The cytokines and the growth factors, such as IL-6, M-CSF, IL-10, HGF, TGF-β and PGE2 contribute to preventing apoptosis of injured pancreatic β-cells and enhancing regeneration of endogenous progenitor cells via angiogenic, cytoprotective, anti-inflammatory, mitogenic and anti-apoptotic effects (21).

It was reported that mitochondria use oxidative phosphorylation to convert dietary intake into ATP; in the process, they generate ROS, which can damage mitochondrial DNA, impair respiratory chain function, and cause nuclear DNA damage and cellular checkpoint activation (27). p53 is a transcription factor that plays a key role in both cell cycle arrest and apoptosis. p53 has many anticancer mechanisms and plays a role in apoptosis, genetic stability, and inhibition of senescence/apoptosis (28).

Present study was to investigate the potential molecular signaling pathways of UVA-induced HDF senescence engaged by HAMSCs. We found that HAMSCs promoted proliferation in UVA induced HDFs which confirmed by flow cytometry. SA-β-gel staining revealed that senescence of UVA irradiated HDFs co-cultured with HAMSCs decreased compared with HDFs accepted UVA irradiation only. ROS generation in UVA induced HDFs was determined to measure the anti-oxidant properties. The excessive production of ROS, such as superoxides and H2O2 severely damages the DNA, protein and lipids. Our findings suggest that HAMSCs inhibited ROS generation in UVA-induced HDFs. Expression of MMP, p53, p38, SIRT1 were also significantly increased in the co-culture group. By improving senescence against oxidative stress, HAMSCs might represent an appropriate therapeutic alternative against UVA induced skin aging.

Signal pathways involved in oxidative stress-induced inhibition of senescence consist of MAPK, Akt/mTOR/4EBP1, p53 and NFκB [Sreedhar et al (29), 2016]. The present study highlights the antioxidant role of HAMSCs in promoting UVA-induced proliferation and senescence. We found that activation of the ERK/MAPK signaling pathway is essential for protective effect against oxidative stress induced cell injury in HDFs. These data shed light on the molecular mechanism the signaling cascade mediated by HAMSCs and identify the potential role of HAMSCs in tissue engineering.

Acknowledgements

The present study was support by the Nanjing Medical Science and Technology Development Fund Project (grant no. 2015NJMUZD088).

References