Pulmonary arterial hypertension is characterized by increased thickness of pulmonary vessel walls due to both increased proliferation of pulmonary arterial smooth muscle cell (PASMC) and deposition of extracellular matrix. In patients suffering from pulmonary arterial hypertension, endothelin-1 (ET-1) synthesis is up-regulated and may increase PASMC activity and vessel wall remodeling through transforming growth factor beta-1 (TGF-β1) and connective tissue growth factor.
To assess the signaling pathway leading to ET-1 induced proliferation and extracellular matrix deposition by human PASMC.
PASMC were serum starved for 24 hours before stimulation with either ET-1 and/or TGF-β1. ET-1 was inhibited by Bosentan, ERK1/2 mitogen activated protein kinase (MAPK) was inhibited by U0126 and p38 MAPK was inhibited by SB203580.
ET-1 increased PASMC proliferation when combined with serum. This effect involved the mitogen activated protein kinases (MAPK) ERK1/2 MAPK and was abrogated by Bosentan which caused a G1- arrest through activation of p27(Kip). Regarding the contribution of extracellular matrix deposition in vessel wall remodeling, TGF-β1 increased the deposition of collagen type-I and fibronectin, which was further increased when ET-1 was added mainly through ERK1/2 MAPK. In contrast, collagen type-IV was not affected by ET-1. Bosentan dose-dependently reduced the stimulatory effect of ET-1 on collagen type-I and fibronectin, but had no effect on TGF-β1.
Conclusion and Clinical Relevance
ET-1 alone does not induce PASMC proliferation and extracellular matrix deposition. However, ET-1 significantly up-regulates serum induced proliferation and TGF-β1 induced extracellular matrix deposition, specifically of collagen type-I and fibronectin. The synergistic effects of ET-1 on serum and TGF-β1 involve ERK1/2 MAPK and may thus present a novel mode of action in the pathogenesis of pulmonary arterial hypertension.
Citation: Lambers C, Roth M, Zhong J, Campregher C, Binder P, Burian B, et al. (2013) The Interaction of Endothelin-1 and TGF-β1 Mediates Vascular Cell Remodeling. PLoS ONE 8(8): e73399. https://doi.org/10.1371/journal.pone.0073399
Editor: Nikolaos Frangogiannis, Albert Einstein College of Medicine, United States of America
Received: February 18, 2013; Accepted: July 19, 2013; Published: August 28, 2013
Copyright: © 2013 Lambers et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was supported by an unrestricted grant of Actelion Pharmaceuticals to L.-H.B. and by an unrestricted research grant by the G & J Bangerter-Rhyner Stiftung (#8427/HEG-DSV) to M.R. The funders had no role in the study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have the following interests. This study was partly supported by an unrestricted grant from Actelion Pharmaceuticals. C.L. has received a travel grant from Actelion Pharmaceuticals. The Bosentan used in this study is an Actelion Pharmaceuticals product. There are no further patents, products in development or marketed products to declare. This does not alter the authors' adherence to all the PLOS ONE policies on sharing data and materials, as detailed online in the guide for authors.
Pulmonary arterial hypertension (PAH) is characterized by the progressive increase of pulmonary vascular resistance and pulmonary arterial pressure, leading to right heart failure and death [1,2]. PAH is either a disease on its own or occurs as co-morbidity in patients suffering from hypoxia, scleroderma, or chronic obstructive pulmonary disease (COPD) [2,3]. A major pathology of PAH is the structural change of the pulmonary arterial vessel wall, which is expressed as hypertrophic smooth muscle and increased deposition of extracellular matrix (ECM) in the tunica media [4,5]. Both events are independent of each other and result in the narrowing of the lumen of pulmonary arteries. The thickened vessel wall is caused by increased deposition of ECM and by smooth muscle hyperplasia/hypertrophy; together these pathologies reduce the flexibility of the vessel wall and increase the constrictive force of the muscle bundles, thereby increasing the pulmonary arterial blood pressure .
Endothelin-1 (ET-1) plasma levels are prominently increased in PAH patients and correlate with pulmonary vascular resistance, pulmonary arterial pressure, cardiac index, and cardiac output [6,7]. ET-1 binds and activates the G-protein coupled ETA and ETB receptors and thereby increase intracellular calcium levels, which in turn activate both phospholipase C and protein kinase C [8–11]. Both ET-receptors mediate vasoconstriction and stimulate pulmonary arterial smooth muscle cell (PASMC) proliferation [10–12]. The mechanism underlying the ET-1 dependent thickening of the pulmonary arterial wall involves the increase of intracellular calcium, cAMP generation and subsequent up-regulation of cyclo-oxygenase 2 in an autocrine loop . There is evidence that the distribution of the ET-receptors is cell type and species-specific; therefore, data obtained in PAH animal models cannot be directly compared to the pathology of human PAH .
In human lung fibroblasts and vascular smooth muscle cells, ET-1 activates at least one mitogen-activated protein kinases (MAPK), ERK1/2, which in turn activates cyclins and cyclin-dependent kinases resulting in cell proliferation and subsequently PASMC hyperplasia in PAH [15,16]. MAPK also mediate the increase of ECM deposition in the vessel wall of PAH patients [17,18]. Moreover, PAH is associated with an altered interaction of MAPK with the transforming growth factor β1 (TGF-β1) activated signaling cascades, which are relevant to ECM restructuring [17,19]. Increased expression of TGF-β1 and connective tissue growth factor (CTGF) have been observed in PAH vessel and contribute to PASMC growth and collagen deposition [17,20]. Taking into account that the collagen content of pulmonary arteries has been suggested as an indicator of PAH staging and progression, the role of TGF-β1 and CTGF, together with other disease relevant stimuli, such as ET-1 on this pathology, has to be further investigated . However, it is not known which specific components of the ECM participate in PAH vessel wall remodeling.
In this study, we determined the effect of ET-1 alone as well as in combination with a ubiquitous mitogen and TGF-β1 on human primary PASMC. We determined the contribution of ET-1 and its receptors on TGF-β1 induced MAPK signaling, proliferation and ECM metabolism in human primary PASMC.
Materials and Methods
Cell culture and proliferation
Experiments were performed using a commercially available cell line of primary human PASMC (CC-2581, Cambrex-Bioscience, Walkersville, USA), which was grown as recommended by the manufacturer. Experiments were performed when the monolayer of PASMC reached 70%-80% confluence. Prior to experiments, PASMC were serum-deprived in medium containing 0.5% fetal calf serum (FCS) for 24 hours. ET-1 (Sigma, Vienna, Austria) was used in a concentration range of 0.01-1 µM. Bosentan (Tracleer™, Actelion Pharmaceuticals, Allschwil, Switzerland) was used at 10 and 100 µM and was added to cell cultures 15 minutes before stimulation. FCS (5%) was used as a positive control.
Cell proliferation was determined by direct cell count after 3 days of incubation .
PASMC were grown on chamber slides and treated with ET-1 and/or Bosentan for various time periods before fixation in methanol (15 minutes). Slides were washed 3x with phosphate buffered saline (PBS), then incubated with blocking buffer (10% BSA in PBS) for 20 minutes at room temperature (RT), followed by incubation (2 hours, RT) with a monoclonal antibody specific to phosphorylated amino acids Thr 202 and Tyr 204 of ERK1/2 (#9106, diluted 1:400, Cell Signaling Technology, USA). Slides were washed 5x with PBS and incubated (45 minutes, RT) with a FITC-conjugated species specific second antibody (Sigma). Propidium iodide (15 minutes) was used to stain nuclei. Slides were washed 3x with blocking buffer and evaluated by fluorescence microscope (Olympus, BX41, Vienna, Austria).
Proteins: Whole cell, nuclear and cytosolic
PASMC were harvested in ice cold PBS and centrifuged (1000xg, 6 minutes). Whole cell lysates where prepared by resuspension of the cell pellet in lysis buffer [50 mM/L TrisCl pH 7.4, 150 mM NaCl, 1mM EDTA pH 8, 1% NP-40, complete protease inhibitor cocktailTM (Roche Diagnostics, Vienna, Austria)] and frozen twice in liquid nitrogen and incubated on ice (20 minutes). The supernatant was collected after centrifugation (13,000×g, 15 minutes, 4°C).
Cytoplasmic proteins were extracted from cells in low-salt buffer (20 mM HEPES pH 7.9, 10 mM KCl, 1 mM EDTA, 1 mM EGTA, 0.2% NP-40, 10% glycerol complete protease inhibitorTM (Roche Diagnostics, Vienna, Austria) and incubated on ice for 10 minutes. After centrifugation (13,000xg, 1 minute, 4°C), the supernatant was collected as cytosolic protein fraction. The remaining pellet was dissolved in high-salt buffer (420 mM NaCl, 20 mM HEPES pH 7.9, 10 mM KCl, 1 mM EDTA, 1 mM EGTA, 20% glycerol, Complete Protease Inhibitor™) and incubated on ice (30 minutes), followed by centrifugation (13,000xg, 10 minutes, 4°C). The supernatant was collected as nuclear protein fraction. Protein concentrations were determined by Bradford assay (Bio-Rad, Vienna, Austria) at 595 nm. In experiments for protein phosphorylation studies, we added PhosSTOP buffer (Roche Diagnostics) to protein samples.
Proteins (25 μg) were size fractionated by gel electrophoresis (12% SDS-polyacrylamide gel), then transferred onto a PVDF membrane (Millipore Corp., Billerica, USA) by standard protocols. The transfer was confirmed by Ponceau red staining . Membranes were incubated (2 hours, RT) in blocking buffer (PBS, 0.1% Tween-20, 5% skimmed milk) before a protein-specific monoclonal antibody was added for overnight incubation (4°C). The membranes were washed 3x (80 nM Na2HPO4, 20 mM NaH2PO4, 100 mM NaCl, 0.1% Tween-20, pH 7.5) and then incubated (90 minutes, RT) with a secondary horse radish peroxidase-labeled species specific antibody (Amersham, Buckinghamshire, UK). After being washed 3x with PBS, the protein bands were visualized by enhanced chemiluminescence substrate (Pierce, Illinois, USA) and documented on X-ray film for image analysis (ImageJ version 1.37). Antibodies used: ETA receptor (N-15, Santa Cruz), ETB receptor (A-20, Santa Cruz), actin (Sigma, A-2066), p27(Kip1) (AB3003, Chemicon).
ECM, collagen and fibronectin deposition
Deposition of total ECM was determined in confluent cell layers. For total ECM, cells were starved for 24 hours before being stimulated with either ET-1 or TGF-β1 for 48 hours. [3H]-proline (1 μM Ci) was added for the last 24 hours before cells were washed with PBS followed by fixation in ice cold methanol: acetic acid (3:1) for 5 minutes and subsequent measuring of ECM incorporated tritium as described earlier .
The deposition of collagen type-I, -III and -IV were determined by a modified enzyme linked immunosorbent assay as described earlier . In brief, PASMC were seeded into a 96-well plate and grown to confluence before being stimulated with ET-1 (1 µM) for 48 and 72 hours. Cells were removed by 1 hour incubation in hypotonic ammonium hydroxide. Plates were incubated with 2% bovine serum albumin (30 minutes), followed by overnight incubation (4oC) with one of the primary anti-bodies (collagen type-I: sc-59772, type-III: sc-8781, type-IV: sc-52317, fibronectin: sc-271098; all from Santa Cruz Biotech (Santa Cruz, USA)). Plates were washed 5x with PBS and incubated with a secondary horse radish peroxidase labeled species specific antibody (1 hour, RT). Plates were washed 5x with PBS and 100 μl of TMB solution were applied to each well for 30 minutes. The signal was determined by ELISA reader.
For experiments with neutralizing antibodies targeting pan-TGF-β and CTGF (R&D systems, Abingdon, UK), cells were pre-incubated for 30 minutes before stimulation.
Total mRNA was isolated by TRIZOL  and transcribed into cDNA by reverse transcriptase (Advantage RT-for-PCR Kit, Clontech, Palo Alto, USA). Real-time PCR was performed by LightCycler480 (Roche Diagnostics) using the following commercially available primers: p27(Kip1) mRNA (Hs00153277_m1), TGF-β1(Hs00171257_m1) and collagen type 1 alpha1 chain (Hs01076777_m1); all were purchased as TaqMan pre-developed gene expression assay (Applied Biosystems, ABI, CA, USA). The internal control for PCR analysis was 18S mRNA (Applied Biosystems). 50 PCR cycles (95°C for 10 seconds; 65°C for 30 seconds; 72°C for 5 seconds) were performed. Relative mRNA expression was determined using the ΔCT method .
Cell cycle phase characterization
PASMC (1 x 105 cells/ml) were grown in 6-well plates and stimulated by ET-1 (0.1-1 µM) in the presence or absence of Bosentan (100 µM) for various time intervals. FCS (5%) was used as positive control. Cells were harvested after 6 and 24 hours by accutase treatment, washed with PBS, and fixed in 100% ethanol (30 minutes, on ice). Cells were centrifuged (1500 rpm, 5 minutes) and re-suspended in PBS-containing 20 µg/ml propidium iodide (Sigma) and 60 µg/ml RNase A (Sigma) for 15 minutes (RT). The DNA content was determined by flow cytometry, and the cell cycle distribution was analyzed by CellQuest Software (Becton Dickinson, Mountain View, CA).
Data are presented as mean ± S.E.M. and the Null-hypothesis was: no difference between treated and untreated cells. Protein expression and mRNA transcription were compared by Student’s t-test (two-tailed, unpaired). The effect of Bosentan on ET-1 induced cell cycle progression was compared by multivariate analysis ANOVA. Results were considered significant when the p-value was < 0.05.
Effects of endothelin-1 on cell proliferation
ET-1 (0.1-1 μM) did not induce proliferation of growth arrested, serum starved PASMC; while 5% FCS stimulation increased the cell number by ~1.8 fold over 3 days (Figure 1A). When combined, ET-1 dose-dependently further increased the FCS (5%) induced proliferation of PASMC up to 1.43 fold (Figure 1B). Bosentan (100 μM) significantly reduced the ET-1 induced proliferation of PASMCs (Figure 1C). The p38 MAPK inhibitor SB203580 (10 µM) had no significant effect on ET-1 induced PASMC proliferation, while the ERK1/2 inhibitor U0126 significantly reduced both ET-1 and 5% FCS-induced proliferation (Figure 1C). To further characterize the effect of ET-1 on proliferation control, we determined the cell cycle distribution and found that ET-1 reduced the number of cells in the G1-phase in a dose-dependent manner, while it increased the number of cells in G2-phase from 39.2% to 48.6%. When pre-incubated with Bosentan, the percentage of cells in the G2-phase significantly decreased to 33.5% (Figure 1D). The inhibitory effect of Bosentan on ET-1 induced proliferation was paralleled by increased nuclear accumulation of the cell cycle inhibitor p27(Kip1) (Figure 1E) while p21(Waf1/Cip1) was not affected (data not shown). TGF-ß (0, 0.5, 1 and 5 ng/ml) had no effect on proliferation (data only shown for 5 ng/ml, Figure 1F). In contrast, the addition of ET-1 (10 nM) significantly induced proliferation, while the ERK1/2 inhibitor U0126 significantly reduced the combined effect of ET-1 and TGF-ß-induced proliferation (Figure 1F).
(A) ET-1 alone has no mitogenic effect, while 5% foetal calf serum (FCS) induced proliferation of PASMC within 3 days (n = 6). (B) When combined with 5% FCS, ET-1 dose-dependently increased cell numbers within 3 days (n = 6). Similar results were obtained after 5 days. (C) ET-receptor blockade by Bosentan and chemical Erk1/2 MAPK inhibition abolished the supportive effect of ET-1 on serum-induced PASMC proliferation (n = 3). (D) ET-1 induced accumulation of S/G2-phase cells is prevented by Bosentan (n = 3). (A–D) Bars represent mean ± SEM. (E) Representative immune-blot of the effect of ET-1 and Bosentan on cell compartment distribution of p27(Kip), similar results were obtained in 3 additional experiments. (F) TGF-ß alone did not induce proliferation, whereas the addition of ET-1 significantly increased PASMC proliferation, which was abolished by the inhibition of Erk1/2 MAPK.
The role of ERK1/2 MAP-Kinase in ET-1 induced proliferation
In human PASMC, 5% FCS significantly induced the phosphorylation of ERK1/2 MAPK by 1.9 fold at 60 minutes; while the content of total ERK1/2 MAPK was not changed (Figure 2A). Addition of ET-1 to 5% FCS further increased the phosphorylation of ERK1/2 MAPK, and this effect of ET-1 was prevented by 30 minutes pre-incubation with Bosentan (Figure 2A). In the presence of U0126, the phosphorylation of ERK1/2 MAPK was completely suppressed (Figure 2A). The results from triplicate experiments for all conditions were quantified by image analysis and are presented as bar charts in Figure 2B. The nuclear accumulation of ERK1/2 in the presence of ET-1 has also been demonstrated by immune-fluorescence microscopy (Figure 2C).
(A) Representative immune-blot of Erk1/2 MAPK phosphorylation (phos-Erk1, phos-Erk2). ET-1 and 5% FCS activate phosphorylation of Erk1/2 MAPK, and Bosentan prevents the additive effect of ET-1 dependent Erk1 and Erk2 phosphorylation, while the Erk172 inhibitor U0126 prevents all Erk1/2 phosphorylation. Similar experiments were performed in three additional experiments, and the result of all four experiments are presented as bar chart (mean ± SEM) in panel B. (C) The ET-1 supportive effect on serum induced nuclear accumulation of Erk1/2MAPK (representative microscopy of 5 different experiments).
ET-1 alters extracellular matrix synthesis through TGF-β1 but not through CTGF
Tissue remodeling in PAH also involves increased ECM deposition. Therefore, we assessed the effect of ET-1 alone or in combination with the fibrosis relevant stimulus TGF-β1 in PASMC. As shown in Figure 3A, ET-1 stimulated the secretion of TGF-β1 by PASMC over 3 days continuously; this effect of ET-1 was prevented when the cells were pre-incubated for 30 minutes with Bosentan. This was confirmed on the mRNA level (Figure 3B). When combined with 5% serum, TGF-β1 mRNA levels were further increased while Bosentan significantly reduced ET-1 and serum induced TGF-β1 mRNA levels as shown in Figure 3B. Regarding the role of MAPK in ET-1 signaling, we provide data in Figure 3C that UO126 but not SB203580 inhibited ET-1 induced TGF-β1 mRNA de novo synthesis. We further observed that ET-1 stimulation increased the secretion of CTGF by PASMC and pre-incubation with Bosentan prevented this effect (Figure 3D).
(A) TGF-β1 secretion by PASMC stimulated with ET-1 (1 μM) over 72 hours (n = 3; mean ± SEM). (B) The effect of ET-1 with and without 5% FCS and the inhibitory effect of Bosentan on TGF-β1 mRNA synthesis over 24 hours (n = 4; mean ± SEM). (C) Erk1/2 but not p38 MAPK, mediates ET-1 induced mRNA synthesis of TGF-β1 by PASMC over 24 hours (n = 4; mean ± SEM). (D) ET-1 induced CTGF secretion over 72 hours (n = 3; mean ± SEM).
Next we determined the effect of ET-1 on ECM deposition. TGF-β1 but not ET-1 dose dependently increased the deposition of total collagens by PASMC within 2 days as shown in Figure 4A. When combined, ET-1 dose dependently increased the collagen stimulating effect of TGF-β1 (Figure 4B). When the cells were pre-incubated with Bosentan, the drug dose dependently prevented the synergistic effect of ET-1 on TGF-β1 dependent collagen deposition, but it had no effect of TGF-β1 itself (Figure 4C).
(A) Dose-dependent effect of 48 hours stimulation with TGF-β1 or ET-1 on total ECM deposition determined by [3H]-proline incorporation over the final 24 hours (n = 4; mean ± SEM). (B) Dose-dependent supportive effect of ET-1 on TGF-β1-induced total ECM deposition over 48 hours demonstrated by two fixed concentrations of TGF-β1 (n = 4; mean ± SEM). (C) Bosentan inhibits the supportive effect of ET-1 on TGF-β1 induced total ECM deposition, but has no effect on TGF-β1-induced ECM (n = 4; mean ± SEM).
We further investigated the effect of ET-1 on ECM composition and we observed a significant dose dependent increase of collagen type-I by both TGF-β1 and ET-1 (Figure 5A). When combined, the two stimuli had an additive effect on collagen type-I deposition, which was dose dependent for ET-1 (Figure 5B). This additive effect of ET-1 on collagen type-I deposition was dose dependently reduced when the cells were pre-incubated with Bosentan (Figure 5C).
(A) Dose-dependency of TGF-β1 and ET-1 on collagen type-I deposition at 48 hours (n = 4; mean ± SEM). (B) The supportive effect of ET-1 on TGF-β1-induced collagen type-I deposition (n =4; mean ± SEM). (C) Bosentan prevents ET-1 support on TGF-β1 induced collagen type-I deposition (n = 4; mean ± SEM). (D) Dose-dependency of TGF-β1 and ET-1 on fibronectin deposition at 24 hours (n = 4; mean ± SEM). (E) ET-1 supports TGF-β1-induced fibronectin deposition (n =4; mean ± SEM). (F) The preventive effect of Bosentan on ET-1- support on TGF-β1 induced fibronectin deposition (n = 4; mean ± SEM).
Fibronectin also contributes to inflammation and was up-regulated significantly in a dose dependent manner by TGF-β1 and ET-1, with the ET-1 being less effective than TGF-β1 (Figure 5D). When the two stimuli were combined, ET-1 synergistically increased the stimulatory effect of TGF-β1 on fibronectin deposition (Figure 5E). Pre-incubation of the cells with Bosentan reduced the synergistic effect of ET-1 on fibronectin deposition; however, the inhibitory efficacy was not as strong as observed for collagen type-I (Figure 5F). We also assessed the effect of ET-1 alone and in combination of TGF-β1 on the deposition of collagen type-IV, which was not significantly affected by ET-1 (Figure 6A).
(A) TGF-β1 but not ET-1 increases collagen type-IV deposition by PASMC (n =4; mean ± SEM). (B) Bosentan inhibits the ET-1 induced de novo synthesis of collagen type-I (n =4; mean ± SEM). (B) The involvement of TGF-β1 and CTGF in ET-1 induced collagen type-I and fibronectin deposition was investigated in the presence of neutralizing anti TGF-β and anti CTGF antibodies over 48 hours (n = 3; mean ± SEM).
The reducing effect of Bosentan on collagen type-I deposition occurs on the transcription level as shown in Figure 6B. Pre-incubation of the cells with either TGF-β1 or CTGF neutralizing antibodies over 24 hours significantly reduced the ET-1 stimulatory effect on collagen type-I and fibronectin. In figure 6C, we provide evidence that the ET-1 induced deposition of collagen type-I was mediated through TGF-β1 alone, while its effect on fibronectin involves both TGF-β1 and CTGF.
Discussion and Conclusions
PASMC play a key role in the pathology of vascular remodeling in PAH. Antagonism of ET-1 receptors is established as one of the most effective PAH therapies . Our study shows that ET-1 has no mitogenic effect on human PASMC. However, in the presence of inflammatory stimuli such as serum, ET-1 increases cell proliferation. Bosentan reduces this ET-1 effect through up-regulation of p27(Kip1). ET-1 increased the de novo synthesis and deposition of collagen type-I involving TGF-β1 and for fibronectin also CTGF. The increase of both ECM components by ET-1 was inhibited by Bosentan. The hypothesis that arterial wall remodeling in PAH results from the supportive effect of ET-1 signaling on that of other mitogens  and on TGF-β1 induced collagen deposition via ERK1/2 MAPK is summarized in Figure 7.
ET-1 alone is a weak inducer of vessel wall remodeling in PAH, but it supports the effect of other mitogens. The supportive effects of ET-1 on vessel wall remodeling involve Erk1/2 MAPK and for ECM deposition TGF-β1 as well as CTGF, but in an ECM component specific mechanisms. We also suggest two major feedback mechanisms: which are activated by ET-1: (a) modified the ECM composition (increased collagen type-I and fibronectin) prepare a vessel wall condition of progressive inflammation; and (b) increased TGF-β1 and collagen type-I stimulate the release of more ET-1 (dotted line: not yet confirmed). The observation that Bosentan or ET-1 receptor blockade abolished all pathological effects of ET-1 suggests that long-term treatment may result in improved symptoms.
Our data show that ET-1 up-regulates PASMC proliferation only in the presence of other mitogens such as serum, which could be used as a model for inflammatory conditions [22,23]. The intracellular signaling pathway that mediates synergistic pro-proliferative effects of ET-1 involves ERK1/2 MAPK, which has been reported earlier to contribute to the remodeling of the neo-intima in different diseases including PAH [11,16,19]. Interestingly, the activation of ERK1/2 MAPK by ET-1 does not occur within minutes, but only becomes significant after 1 hour and lasts over the next 5 hours. The proliferative effect as well as the activation of ERK1/2 MAPK is dependent on ET-1 receptor activity since pre-incubation with Bosentan blocked both effects, which is in line with other studies . Moreover, the activation of ERK1/2 MAPK in vascular smooth muscle cells in particular, was linked to p27(Kip) activation and specific cellular compartmental accumulation [27,28]. In lung tissue, the over-expression of p27(Kip) was associated with attenuated systemic arterial smooth muscle cell proliferation . Our observation that Bosentan inhibits ERK1/2 MAPK activity and increases p27(Kip) expression may explain the observed reduction of vessel wall thickening, which has been documented in clinical studies .
As mentioned above, vessel wall remodeling in PAH consists of two major components, proliferation of tissue forming cells and increase deposition of ECM [17,18,31]. In our experiments, ET-1 increased the de novo synthesis and secretion of both factors, with TGF-β1 preceding that of CTGF, similar to the sequence reported in dermal fibroblasts . In rat vascular smooth muscle cells, though, ET-1 up-regulates CTGF independent of TGF-β1 . Our data indicate that ET-1 alone is insufficient to increase total ECM deposition significantly, but it clearly supported TGF-β1 dependent ECM deposition. However, when combined, ET-1 further enhanced TGF-β1 induced collagen type-I and fibronectin deposition, a similar effect has been reported in fibroblasts where the effect of the combined stimuli was additive . Importantly, the supportive effect of ET-1 on TGF-β1 that we observed on collagen type-I and fibronectin deposition was prevented by Bosentan, which might further explain the reduced vessel remodeling in PAH animal models . We did not observe any supportive effect of ET-1 on TGF-β1-induced collagen type-III nor type-IV deposition. The discrepancy of the stimulatory effect of ET-1 alone on total ECM versus collagen type-I and fibronectin deposition that we observed may be explained by the different methods used. Total ECM deposition was determined by proline incorporation over the last 24 hours of 48 hours stimulation, while the deposition of specific ECM compounds was determined by in house developed ELISAs after 48 hours.
Similar to fibroblasts, the stimulatory effect of ET-1 alone on collagen type-I deposition involved TGF-β1, but not CTGF . In other smooth muscle cell types and different culture conditions, TGF-β1 and CTGF were necessary to up-regulate collagen type-I deposition . In vascular smooth muscle cells, ET-1 induced collagen type-I synthesis was independent of TGF-β1 but dependent on CTGF . The second ECM compound that was up-regulated by ET-1 through TGF-β1 and CTGF was fibronectin, which has recently been reported to be modified in pulmonary hypertension . On the basis of other reports, it can be speculated that an increase of fibronectin in PAH vessels cells may lead to modified interactions between tissue forming cells and immune reactive cells as well as it altered the response of PASMC to neuronal stimuli [37,38]. The importance of the ECM composition in pulmonary arteries to the pathogenesis of PAH has recently been discussed and it was concluded that this might present a marker for the disease progression. However, too little is known on the precise mechanism [29,39]. Such ECM modifications also might present a feedback mechanism to growth factors and hyperplasia as suggested in Figure 7 . Importantly, the pathological effects of ET-1 were all prevented by Bosentan, which is in line with the beneficial anti-remodeling effect of the drug in a clinical study .
In conclusion, our study provides evidence that ET-1 alone is a weak activator of PASMC responses. However, ET-1 significantly supports effects of other PAH relevant stimuli on PASMC responses that could explain PAH vessel wall pathologies. Regarding the therapeutic effect of Bosentan or ET-1 receptors inhibition in general, our data suggests a highly specific beneficial action of the drug.
The authors thank Mrs. Elisabeth Hofbauer for her technical assistance and Mr. C.T. S’ng for preparing the manuscript.
Conceived and designed the experiments: CL MR VP LHB. Performed the experiments: CL MR JZ PB. Analyzed the data: CL MR VP LHB. Contributed reagents/materials/analysis tools: CC BB VP. Wrote the manuscript: CL MR LHB.
- 1. Farber HW, Loscalzo J (2004) Pulmonary arterial hypertension. N Engl J Med 351: 1655-1665. doi:https://doi.org/10.1056/NEJMra035488. PubMed: 15483284.
- 2. Galiè N, Torbicki A, Barst R, Dartevelle P, Haworth S et al. (2004) Guidelines on diagnosis and treatment of pulmonary arterial hypertension. The Task Force on Diagnosis and Treatment of Pulmonary Arterial Hypertension of the European Society of Cardiology. Eur Heart J 25: 2243-2278. doi:https://doi.org/10.1016/j.ehj.2004.09.014. PubMed: 15589643.
- 3. Barberà JA, Blanco I (2009) Pulmonary hypertension in patients with chronic obstructive pulmonary disease: advances in pathophysiology and management. Drugs 69: 1153-1171. doi:https://doi.org/10.2165/00003495-200969090-00002. PubMed: 19537834.
- 4. Humbert M, Montani D, Perros F, Dorfmüller P, Adnot S et al. (2008) Endothelial cell dysfunction and cross talk between endothelium and smooth muscle cells in pulmonary arterial hypertension. Vasc Pharmacol 49: 113-118. doi:https://doi.org/10.1016/j.vph.2008.06.003. PubMed: 18606248.
- 5. Dorfmüller P, Humbert M, Capron F, Müller KM (2003) Pathology and aspects of pathogenesis in pulmonary arterial hypertension. Sarcoidosis Vasc Diffuse Lung Dis 20: 9-19. PubMed: 12737275.
- 6. Galié N, Manes A, Branzi A (2004) The endothelin system in pulmonary arterial hypertension. Cardiovasc Res 61: 227-237. doi:https://doi.org/10.1016/j.cardiores.2003.11.026. PubMed: 14736539.
- 7. Rubens C, Ewert R, Halank M, Wensel R, Orzechowski HD et al. (2001) Big endothelin-1 and endothelin-1 plasma levels are correlated with the severity of primary pulmonary hypertension. Chest 120: 1562-1569. doi:https://doi.org/10.1378/chest.120.5.1562. PubMed: 11713135.
- 8. Schiffrin EL, Touyz RM (1998) Vascular biology of endothelin. J Cardiovasc Pharmacol 32: S2-13. PubMed: 9883741.
- 9. Yanagisawa M, Kurihara H, Kimura S, Tomobe Y, Kobayashi M et al. (1988) A novel potent vasoconstrictor peptide produced by vascular endothelial cells. Nature 332: 411-415. doi:https://doi.org/10.1038/332411a0. PubMed: 2451132.
- 10. Davie N, Haleen SJ, Upton PD, Polak JM, Yacoub MH et al. (2002) ET(A) and ET(B) receptors modulate the proliferation of human pulmonary artery smooth muscle cells. Am J Respir Crit Care Med 165: 398-405. doi:https://doi.org/10.1164/ajrccm.165.3.2104059. PubMed: 11818328.
- 11. Panettieri RA Jr., Goldie RG, Rigby PJ, Eszterhas AJ, Hay DW (1996) Endothelin-1-induced potentiation of human airway smooth muscle proliferation: an ETA receptor-mediated phenomenon. Br J Pharmacol 118: 191-197. doi:https://doi.org/10.1111/j.1476-5381.1996.tb15385.x. PubMed: 8733595.
- 12. Yang Z, Krasnici N, Lüscher TF (1999) Endothelin-1 potentiates human smooth muscle cell growth to PDGF: effects of ETA and ETB receptor blockade. Circulation 100: 5-8. doi:https://doi.org/10.1161/01.CIR.100.1.5. PubMed: 10393673.
- 13. Deacon K, Knox AJ (2010) Endothelin-1 (ET-1) increases the expression of remodeling genes in vascular smooth muscle through linked calcium and cAMP pathways: role of a phospholipase A(2)(cPLA(2))/cyclooxygenase-2 (COX-2)/prostacyclin receptor-dependent autocrine loop. J Biol Chem;285: 25913-25927. doi:https://doi.org/10.1074/jbc.M110.139485. PubMed: 20452970.
- 14. Fukuroda T, Kobayashi M, Ozaki S, Yano M, Miyauchi T et al. (1994) Endothelin receptor subtypes in human versus rabbit pulmonary arteries. J Appl Physiol 76: 1976-1982. PubMed: 8063659.
- 15. Gallelli L, Pelaia G, D’Agostino B, Cuda G, Vatrella A et al. (2005) Endothelin-1 induces proliferation of human lung fibroblasts and IL-11 secretion through an ET(A) receptor-dependent activation of MAP kinases. J Cell Biochem 96: 858-868. doi:https://doi.org/10.1002/jcb.20608. PubMed: 16149067.
- 16. Yogi A, Callera GE, Montezano AC, Aranha AB, Tostes RC et al. (2007) Endothelin-1, but not Ang II, activates MAP kinases through c-Src independent Ras-Raf dependent pathways in vascular smooth muscle cells. Arterioscler Thromb Vasc Biol 27: 1960-1967. doi:https://doi.org/10.1161/ATVBAHA.107.146746. PubMed: 17569879.
- 17. Budd DC, Holmes AM (2012) Targeting TGFβ superfamily ligand accessory proteins as novel therapeutics for chronic lung disorders. Pharmacol Ther 135: 279-291. doi:https://doi.org/10.1016/j.pharmthera.2012.06.001. PubMed: 22722064.
- 18. Jonigk D, Golpon H, Bockmeyer CL, Maegel L, Hoeper MM et al. (2011) Plexiform lesions in pulmonary arterial hypertension composition, architecture, and microenvironment. Am J Pathol 179: 167-179. doi:https://doi.org/10.1016/j.ajpath.2011.03.040. PubMed: 21703400.
- 19. West J (2010) Cross talk between Smad, MAPK, and actin in the etiology of pulmonary arterial hypertension. Adv Exp Med Biol 661: 265-278. doi:https://doi.org/10.1007/978-1-60761-500-2_17. PubMed: 20204736.
- 20. Rodriguez-Vita J, Ruiz-Ortega M, Rupérez M, Esteban V, Sanchez-López E et al. (2005) Endothelin-1, via ETA receptor and independently of transforming growth factor-beta, increases the connective tissue growth factor in vascular smooth muscle cells. Circ Res 97: 125-134. doi:https://doi.org/10.1161/01.RES.0000174614.74469.83. PubMed: 15976312.
- 21. Egito ES, Aiello VD, Bosisio IB, Lichtenfels AJ, Horta AL et al. (2003) Vascular remodeling process in reversibility of pulmonary arterial hypertension secondary to congenital heart disease. Pathol Res Pract 199: 521-532. doi:https://doi.org/10.1078/0344-0338-00457. PubMed: 14533936.
- 22. Yang JQ, Rüdiger JJ, Hughes JM, Goulet S, Gencay-Cornelson MM et al. (2008) Cell density and serum exposure modify the function of the glucocorticoid receptor C/EBP complex. Am J Respir Cell Mol Biol 38: 414-422. doi:https://doi.org/10.1165/rcmb.2007-0079OC. PubMed: 17989362.
- 23. Goulet S, Bihl MP, Gambazzi F, Tamm M, Roth M (2007) Opposite effect of corticosteroids and long-acting beta(2)-agonists on serum- and TGF-beta(1)-induced extracellular matrix deposition by primary human lung fibroblasts. J Cell Physiol 210: 167-176. doi:https://doi.org/10.1002/jcp.20836. PubMed: 17013807.
- 24. Johnson PR, Black JL, Carlin S, Ge Q, Underwood PA (2000) The production of extracellular matrix proteins by human passively sensitized airway smooth-muscle cells in culture: the effect of beclomethasone. Am J Respir Crit Care Med 162: 2145-2151. doi:https://doi.org/10.1164/ajrccm.162.6.9909111. PubMed: 11112129.
- 25. Lambers C, Burian B, Binder P, Ankersmit HJ, Wagner C, Müller M, Zeitlinger M (2010) Early immunomodulatory effects of linezolid in a human whole blood endotoxin model. Int J Clin Pharmacol 48: 419-424.
- 26. Livak KJ, Schmittgen TD (2001) Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods 25: 402-408. doi:https://doi.org/10.1006/meth.2001.1262. PubMed: 11846609.
- 27. Castro C, Díez-Juan A, Cortés MJ, Andrés V (2003) Distinct regulation of mitogen-activated protein kinases and p27Kip1 in smooth muscle cells from different vascular beds. A potential role in establishing regional phenotypic variance. J Biol Chem 278: 4482-4490. doi:https://doi.org/10.1074/jbc.M204716200. PubMed: 12477734.
- 28. Liu AJ, Ling F, Wang D, Wang Q, Lü XD et al. (2011) Fasudil inhibits platelet-derived growth factor-induced human pulmonary artery smooth muscle cell proliferation by up-regulation of p27kip¹ via the ERK signal pathway. Chin Med J (Engl) 124: 3098-3104. PubMed: 22040563.
- 29. Fouty BW, Grimison B, Fagan KA, Le Cras TD, Harral JW et al. (2001) p27(Kip1) is important in modulating pulmonary artery smooth muscle cell proliferation. Am J Respir Cell Mol Biol 25: 652-658. doi:https://doi.org/10.1165/ajrcmb.25.5.4592. PubMed: 11713109.
- 30. Choudhary G, Troncales F, Martin D, Harrington EO, Klinger JR (2011) Bosentan attenuates right ventricular hypertrophy and fibrosis in normobaric hypoxia model of pulmonary hypertension. J Heart Lung Transplant 30: 827-833. doi:https://doi.org/10.1016/j.healun.2011.03.010. PubMed: 21550822.
- 31. Ma W, Han W, Greer PA, Tuder RM, Toque HA et al. (2011) Calpain mediates pulmonary vascular remodeling in rodent models of pulmonary hypertension, and its inhibition attenuates pathologic features of disease. J Clin Invest 121: 4548-4566. doi:https://doi.org/10.1172/JCI57734. PubMed: 22005303.
- 32. Weis MA, Hudson DM, Kim L, Scott M, Wu JJ, Eyre DR (2010) Location of 3-hydroxyproline residues in collagen types I, II, III, and V/XI implies a role in fibril supramolecular assembly. J Biol Chem 285: 2580-2590. doi:https://doi.org/10.1074/jbc.M109.068726. PubMed: 19940144.
- 33. Horstmeyer A, Licht C, Scherr G, Eckes B, Krieg T (2005) Signalling and regulation of collagen I synthesis by ET-1 and TGF-beta1. FEBS J 272: 6297-3309. doi:https://doi.org/10.1111/j.1742-4658.2005.05016.x. PubMed: 16336267.
- 34. Johnson PR, Burgess JK, Ge Q, Poniris M, Boustany S et al. (2006) Connective tissue growth factor induces extracellular matrix in asthmatic airway smooth muscle. Am J Respir Crit Care Med 173: 32-41. doi:https://doi.org/10.1164/rccm.200406-703OC. PubMed: 16179645.
- 35. Rodriguez-Vita J, Ruiz-Ortega M, Rupérez M, Esteban V, Sanchez-López E et al. (2005) Endothelin-1, via ETA receptor and independently of transforming growth factor-beta, increases the connective tissue growth factor in vascular smooth muscle cells. Circ Res 97: 125-134. doi:https://doi.org/10.1161/01.RES.0000174614.74469.83. PubMed: 15976312.
- 36. Wei L, Warburton RR, Preston IR, Roberts KE, Comhair SA et al. (2012) Serotonylated fibronectin is elevated in pulmonary hypertension. Am J Physiol Lung Cell Mol Physiol 302: L1273-L1279. doi:https://doi.org/10.1152/ajplung.00082.2012. PubMed: 22523280.
- 37. Li M, Cui T, Mills DK, Lvov YM, McShane MJ (2005) Comparison of selective attachment and growth of smooth muscle cells on gelatin- and fibronectin-coated micropatterns. J Nanosci Nanotechnol 5: 1809-1815. doi:https://doi.org/10.1166/jnn.2005.436. PubMed: 16433414.
- 38. Olenych SG, Moussallem MD, Salloum DS, Schlenoff JB, Keller TC (2005) Fibronectin and cell attachment to cell and protein resistant polyelectrolyte surfaces. Biomacromolecules 6: 3252-3258. doi:https://doi.org/10.1021/bm050298r. PubMed: 16283753.
- 39. Tabima DM, Roldan-Alzate A, Wang Z, Hacker TA, Molthen RC et al. (2012) Persistent vascular collagen accumulation alters hemodynamic recovery from chronic hypoxia. J Biomech 45: 799-804. doi:https://doi.org/10.1016/j.jbiomech.2011.11.020. PubMed: 22183202.