Open Access

Knockout of endothelin type B receptor signaling attenuates bleomycin-induced skin sclerosis in mice

  • Kengo Akashi1,
  • Jun Saegusa1,
  • Sho Sendo1,
  • Keisuke Nishimura1,
  • Takuya Okano2, 3,
  • Keiko Yagi2,
  • Masashi Yanagisawa4,
  • Noriaki Emoto2, 3 and
  • Akio Morinobu1Email author
Arthritis Research & Therapy201618:113

https://doi.org/10.1186/s13075-016-1011-4

Received: 16 December 2015

Accepted: 3 May 2016

Published: 21 May 2016

Abstract

Background

Endothelin-1 (ET-1) is important in the pathogenesis of systemic sclerosis (SSc). ET-1 binds two receptors, endothelin type A (ETA) and endothelin type B (ETB). Dual ETA/ETB receptor antagonists and a selective ETA receptor antagonist are used clinically to treat SSc, and the effect of these antagonists on fibroblast activation has been described. However, the role of ETB receptor signaling in fibrogenesis is less clear. This study was conducted to evaluate the profibrotic function of ETB receptor signaling in a murine model of bleomycin (BLM)-induced scleroderma.

Methods

We used ETB receptor–knockout (ETBKO) mice, which are genetically rescued from lethal intestinal aganglionosis by an ETB receptor transgene driven by the human dopamine β-hydroxylase (DβH)-gene promoter, and wild-type mice with DβH-ETB (WT). BLM or phosphate-buffered saline (PBS) was administered subcutaneously by osmotic minipump, and skin fibrosis was assessed by dermal thickness, subcutaneous fat atrophy, and myofibroblast count in the dermis. Dermal fibroblasts isolated from ETBKO and WT mice were cultured in vitro, stimulated with BLM or ET-1, and the expression of profibrotic genes was compared by quantitative PCR.

Results

Dermal thickness, subcutaneous fat atrophy, and myofibroblast counts in the dermis were significantly reduced in ETBKO mice compared to WT mice, after BLM treatment. Compared with wild-type, dermal fibroblasts isolated from ETBKO mice showed lower gene expressions of α-smooth muscle actin and collagen 1α1 in response to BLM or ET-1 stimulation in vitro.

Conclusions

ET-1–ETB receptor signaling is involved in skin sclerosis and in collagen synthesis by dermal fibroblasts.

Keywords

Systemic sclerosis Endothelin type B receptor Dermal fibroblast

Background

Systemic sclerosis (SSc), a connective-tissue disease of unknown etiology, is characterized by autoimmunity, microvascular impairment, chronic inflammation, and fibrotic changes in the skin and internal organs [1]. The pathogenesis of SSc has been studied in a bleomycin (BLM)-induced scleroderma model [2, 3]. Among fibrotic agents known to contribute to scleroderma, the role of endothelin-1 (ET-1) in SSc fibrosis has been well described [4]. The plasma concentration of ET-1 is elevated in SSc patients, and endothelin receptor expression is increased in the lungs and skin [5, 6]. ET-1 plays an important role in murine model of BLM-induced scleroderma because endothelin receptor antagonist therapy is reported to attenuate skin fibrosis of mice [4]. Recently, vascular endothelial cell-specific ET-1 knockout mice are also reported to attenuate skin sclerosis [7]. ET-1, which was first characterized as a potent vasoconstrictive peptide derived from endothelial cells, is an important profibrotic mediator that induces the differentiation of fibroblasts to myofibroblasts and increases the extracellular matrix. Therefore, ET-1 plays a critical role in vascular impairment and fibrosis in SSc patients.

ET-1 binds two receptor subtypes, the endothelin type A (ETA) and endothelin type B (ETB) receptors [8]. Treatment with a dual ETA/ETB receptor antagonist or a selective ETA receptor antagonist improves mortality in patients with pulmonary arterial hypertension [911]. ETA receptor signaling is critical for dermal fibroblast activation [12]. However, the role of ETB receptor signaling in fibrogenesis is less clear.

To investigate the profibrotic activity of the ET-1–ETB receptor signal in fibrosis, we used endogenous ETB receptor–knockout (ETBKO) mice with an ETB receptor transgene driven by the human dopamine β-hydroxylase (DβH) gene promoter, which generated “rescued” ETB-knockout mice [1315]. ETB-receptor mutant mice and general (not rescued) ETBKO mice, which have aganglionic megacolon and white spotting on the coat, die before reaching adulthood because ETB receptor signaling is important in generating melanocytes and enteric neurons [16]. In the “rescued” ETBKO mice, a functional ETB receptor is expressed only in the enteric nervous system; other tissues lack ETB receptors. These mice survive into adulthood [17].

Here we show that ETBKO mice were resistant to BLM-induced scleroderma, and that compared to WT mice, ETBKO mice showed less fibroblast activation and myofibroblast formation in response to BLM or ET-1.

Methods

Animals

The mice were housed in the animal facility of Kobe Pharmaceutical University, with a 12-h dark/light cycle and ad libitum water and food. Heterozygous ETBKO mice (ETB+/-) on a C57BL/6 J genetic background were generated as described previously [17, 18]. The human DβH gene promoter–regulated ETB receptor transgene (DβH-ETB) and ETB+/- with DβH-ETB were generated as described previously [1315]. ETB+/- mice were crossed with DβH-ETB mice to obtain three genotypes: wild-type ETB+/+ with DβH-ETB (WT mice), ETB+/- with DβH-ETB (heterozygous KO mice), and ETB-/- with DβH-ETB (ETBKO mice). The ETBKO mice had a partly white coat that distinguished them from heterozygous KO and WT mice. All experimental protocols were approved by the Ethics Review Committee for Animal Experimentation of Kobe Pharmaceutical University.

Reagents and antibodies

BLM and ET-1 (H-6995) were purchased from Nippon-Kayaku (Tokyo, Japan) and Bachem (Bubendorf, Switzerland), respectively. Dulbecco's modified Eagle's medium (DMEM) (Nissui-Seiyaku, Tokyo, Japan), RPMI 1640 (Wako Pure Chemical Industries, Osaka, Japan), fetal bovine serum (FBS) (MP Biomedicals, Santa Ana, CA, USA), 1 % penicillin–streptomycin (Lonza, Basel, Switzerland), L-glutamine (Thermo Fisher Scientific, Waltham, MA, USA), and type 1 collagenase (Worthington Biochemical Corporation, Lakewood, NJ, USA) were also used. Bovine serum albumin (BSA), 2 M acetic acid, and dispase were purchased from Sigma-Aldrich (St. Louis, MO, USA). For immunohistochemistry experiments, anti-alpha smooth-muscle actin (αSMA) antibody (ab32575), anti-collagen 1 antibody (ab21286), anti-CD3 antibody (ab16669), anti-F4/80 antibody (ab111101) and rabbit polyclonal IgG (ab27472) were purchased from Abcam (Cambridge, UK), and anti-myeloperoxidase antibody (PA5-16672) purchased from Thermo Fisher Scientific (Waltham, MA, USA). A rabbit ABC Staining System (sc-2018) was purchased from Santa Cruz Biotechnology (Dallas, TX, USA).

BLM administration

BLM was dissolved in phosphate-buffered saline (PBS). BLM or PBS was administered with osmotic minipumps according to previous reports with minor modifications [1921]. Briefly, osmotic minipumps (Alzet2001; Durect, Cupertino, CA, USA) containing 200 μl of BLM (125 mg/kg) or PBS were implanted subcutaneously onto the back of WT or ETBKO mice aged 6–10 weeks; this was counted as day 0. The pumps delivered 1.0 μg/h for 7 days. The mice were sacrificed on day 28, and skin and lung tissues were taken. Skin samples were taken a short distance from the osmotic minipump to obtain samples that were not affected by pump implantation.

Histology and immunohistochemistry

The skin and lung samples were fixed in 4 % paraformaldehyde, embedded in paraffin, sectioned, and stained with Masson’s trichrome. To evaluate the BLM-induced scleroderma, we assessed dermal thickening and subcutaneous fat atrophy by measuring the distances between the epidermis and dermis and between the dermis and subcutaneous fat at 40× magnification. The degree of lung fibrosis was quantified using the Ashcroft score at 40× magnification [22]. Collagen 1 deposition area in the dermis was measured with ImageJ software (National Institutes of Health). Fibroblast activation was assessed by αSMA immunohistochemical staining of the skin sections, and αSMA-positive myofibroblasts in the dermis were counted at 100× magnification. To examine whether ETB receptor is involved in the inflammation of this model, we counted myeloperoxidase-positive neutrophils, CD3-positive T lymphocytes and F4/80-positive macrophages in the dermis at 100× magnification.

Collection of bronchoalveolar lavage fluid (BALF)

To evaluate lung inflammation, a cell count of BALF was performed. Immediately after the mice were sacrificed, a 20-gauge intravenous catheter was inserted into the trachea. A total of 0.5 ml of PBS was instilled three times and withdrawn from the lung via an intratracheal cannula. After BALF was centrifuged, the pellet was resuspended in 1 ml of PBS. Total BALF cells were counted with a hemocytometer. The BALF solutions were stained with May-Giemsa staining after cytospin centrifuge, and the white blood cell differentiation was evaluated by morphological criteria using a light microscope.

Murine dermal fibroblast isolation and culture

Dermal fibroblasts were isolated from WT and ETBKO mice at 3–4 weeks of age according to previous reports, with minor modification [23]. Skin samples were placed dermis-down in culture dishes containing RPMI + 3.6 % dispase, and incubated overnight at 4 °C. The dermis was separated from the epidermis, placed in RPMI + 0.05 % type I collagenase, and incubated at 37 °C for 30 min. The cell suspension was filtered through sterile gauze into a 50-mL conical tube. After adding an equal volume of DMEM + 10 % FBS containing penicillin, streptomycin, and L-glutamine, the suspension was centrifuged at 200 × g for 10 min. Fibroblasts were resuspended in DMEM + 10 % FBS, plated in 100-mm culture dishes, and incubated at 37 °C in 5 % CO2 and 95 % room air. For in vitro experiments, fibroblasts were seeded into 6-well plates (1 × 105 per well) and incubated in DMEM + 10 % FBS at 37 °C in 5 % CO2. When the fibroblasts had grown to approximately 80 % confluence, the medium was changed and the fibroblasts were treated with 20 μg/ml BLM or 500 nM ET-1 for 24 h. The BLM was dissolved in DMEM without FBS; the ET-1 was dissolved in 0.1 % acetic acid + 0.01 % BSA.

Quantitative real-time polymerase chain reaction (PCR)

Total RNA was isolated from fibroblasts using an RNeasy Mini kit (Qiagen, Hilden, Germany), followed by cDNA synthesis using a QuantiTect Reverse Transcription kit (Qiagen). PCR reaction mixtures were prepared using the QuantiTect SYBR Green PCR kit (Qiagen), followed by quantitative PCR on a PikoReal system (Thermo Fisher Scientific). The following primer pairs were used: collagen 1α1 (Col1α1), 5’-TGACTGGAAGAGCGGAGAGTACT-3’ (forward) and 5’-GGTCTGACCTGTCTCCATGTTG-3’ (reverse); αSMA, 5’-AGAGACTCTCTTCCAGCCATC-3’ (forward) and 5’-GACGTTGTTAGCATAGAGATC-3’ (reverse); ET-1, 5’-GTGTCTACTTCTGCCACCTGGACAT-3’ (forward) and 5’-GGGCTCGCACTATATAAGGGATGAC-3’ (reverse); endothelin receptor type A (EDNRA), 5’-CCTTATCTSCGTGGTCATTG-3’ (forward) and 5’-ACTGAGAGCACAGAGGTTC-3’ (reverse); endothelin receptor type B (EDNRB), 5’-GGAATCACAGTGCTGAGTC-3’ (forward) and 5’-CTTTGTAGTCCGACGTAATC-3’ (reverse); glyceraldahyde-3-phosphate dehydrogenase (GAPDH), 5’-AACTTTGGCATTGTGGAAGG-3’ (forward) and 5’-ACACATTGGGGGTAGGAACA-3’ (reverse). GAPDH was used as an internal control to normalize the amount of loaded , complementary DNA (cDNA).

Measurement of soluble collagen content

Sircol collagen assay (Biocolor Ltd., Belfast, Northern Ireland) was used to quantify soluble collagen contents in fibroblast culture supernatant according to the manufacturer’s instructions with minor modification. Briefly, 200 μl of supernatant was mixed with 1 ml of Sircol dye reagent for 30 minutes. After centrifugation, the pellets were dissolved in 1 ml Sircol alkali reagent and vortexed. Relative absorbance was measured at 540 nm.

Statistical analysis

Data are presented as mean ± standard error of the mean (SEM). Differences between groups were analyzed by Student’s t test using GraphPad Prism 5 software (GraphPad Software Inc., La Jolla, CA, USA) and p < 0.05 was considered statistically significant.

Results

ETBKO mice resisted BLM-induced scleroderma

WT and ETBKO mice were treated with BLM or PBS by osmotic minipump. No mice died due to the osmotic minipump implantation or BLM administration. To examine the biological significance of ETB receptor signaling after BLM administration, we measured body-weight changes from day 0 to day 28. ETBKO mice were smaller than WT mice of the same age, and ETBKO mice gained less body weight than did WT mice when treated with PBS. However, while BLM-treated WT mice did not gain body weight, BLM-treated ETBKO mice gained weight similarly to the PBS-treated ETBKO mice (Fig 1b).
Fig. 1

Study design and body-weight changes of each mice group after BLM treatment. a Summary of this experimental model and sample number of each group. Osmotic pumps containing 200 μl of BLM (125 mg/kg) or PBS were implanted subcutaneously onto the back of WT or ETBKO mice on day 0. Pumps deliver their contents 1.0 μg/h for 7 days. Mice were sacrificed on day28. b Body-weight changes from day 0 to day 28 in WT and ETBKO mice. The body-weight change was calculated as [(body weight on day 28) − (body weight on day 0)] × (body weight on day 0)-1 × 100 (%). Each dot indicates the body-weight change in an individual mouse (* p < 0.05). BLM bleomycin, DβH-ET B endothelin type B receptor transgene driven by the human dopamine β-hydroxylase gene promoter, ET B KO endothelin type B receptor knockout, PBS phosphate-buffered saline, WT wild-type

To determine the ETB receptor’s role in BLM-induced scleroderma, skin specimens were obtained from each group on day 28 after implanting the osmotic minipump. The skin samples were stained with Masson’s trichrome to evaluate the dermal thickness and subcutaneous fat atrophy. In WT mice, BLM treatment increased the distance between the epidermis and dermis, and reduced the distance between the dermis and subcutaneous fat. In contrast, these distances did not change significantly in the ETBKO mice treated with PBS or BLM (Fig. 2a-c). Likewise, collagen 1 deposition area in the dermis was increased by BLM-treatment in WT mice, but the increment was not seen in ETBKO mice (Fig. 2d). These results suggested that ETB receptor signaling is associated with BLM-induced skin sclerosis. Also lung fibrosis and inflammation were evaluated, but neither cell counts in BALF nor lung histological scores were not significantly different between WT and ETBKO with BLM treatment (Additional file 1: Figure S1).
Fig. 2

ETBKO mice resist BLM-induced skin sclerosis. a Representative images of dermis sections stained with Masson's trichrome at 40× magnification. b Changes in dermal thickness (epidermal–dermal distance) and c subcutaneous fat atrophy (dermal–subcutaneous fat distance) in BLM- or PBS-treated WT and ETBKO mice; values are shown as the mean fold change from PBS-treated WT (WT-PBS) mice. d Collagen 1 deposition area in dermis of each mice group. (* p < 0.05) (n = 5–10 mice per group). BLM bleomycin, ET B KO endothelin type B receptor knockout, PBS phosphate-buffered saline, WT wild-type

Inhibited fibroblast activation protects ETBKO mice against BLM-induced scleroderma

BLM-induced scleroderma is associated with the differentiation of fibroblasts into myofibroblasts. These myofibroblasts, which are identified by αSMA expression, promote fibrosis by producing collagen and other extracellular matrix components [24, 25].

To determine whether ETB receptor signaling contributes to BLM-induced fibroblast differentiation, we counted the number of αSMA-positive cells in the dermis of BLM- or PBS-treated WT and ETBKO mice. BLM increased the number of αSMA-positive myofibroblasts in the WT but not ETBKO dermis, indicating that ETB is involved in myofibroblast formation (Fig. 3).
Fig. 3

Fewer αSMA-expressing myofibroblasts are observed in the dermis of ETBKO than WT mice after BLM treatment. a Representative images showing the immunohistochemical staining of skin samples for αSMA (upper) and isotype (lower) at 100× magnification. Red arrows indicate myofibroblasts (αSMA-expressing spindle-shaped cells). b Average myofibroblast counts per field of view in the dermis, counted at 100× magnification (* p < 0.05); n = 5–10 mice per group. BLM bleomycin, HPF high-power field, ET B KO endothelin type B receptor knockout, PBS phosphate-buffered saline, WT wild-type

Inflammatory cell filtration in the dermis was counted to determine whether the degree of inflammation was different between WT and ETBKO skin fibrosis. The numbers of myeloperoxidase-positive neutrophils, CD3-positive T cells and F4/80-positive macrophages in the dermis were significantly increased when treated with BLM. However, the numbers of these inflammatory cells were not different between WT and ETBKO mice both before and after BLM treatment (Fig. 4).
Fig. 4

Infiltration of inflammatory cells in the dermis of WT and ETBKO mice after BLM treatment. The average cell counts of a myeloperoxidase, b CD3, and c F4/80-positive cells in the dermis. The cells were counted per field of view at 100× magnification; n = 5–10 mice per group. (* p < 0.05). BLM bleomycin, ET B KO endothelin type B receptor knockout, HPF high-power field, PBS phosphate-buffered saline, WT wild-type

Collectively ETB receptor signaling seemed to contribute to fibroblast activation independent of inflammation.

The ETB receptor is associated with dermal fibroblast activation and collagen synthesis in response to BLM or ET-1

Because fibroblasts play a critical role in fibrosis, we next examined the characteristics of dermal fibroblasts from WT and ETBKO mice. ET-1 or BLM stimulation is reported to induce fibroblasts to express profibrotic genes [12, 26]. Thus, we isolated dermal fibroblasts from WT and ETBKO mice and assessed their activation and collagen synthesis in response to ET-1 or BLM in vitro. Dermal fibroblasts from ETBKO mice expressed little or no EDNRB mRNA but expressed EDNRA normally, as expected (Fig. 5a, b).
Fig. 5

Knockout of the ETB receptor signal reduces the activation of skin-derived fibroblasts in response to BLM. a EDNRA and b EDNRB mRNA levels in skin-derived fibroblasts from WT and ETBKO mice (n = 5 each). c-e BLM-induced fibroblast activation in WT and ETBKO mice (n = 6–9 each), determined by the gene expression levels of Col1α1, αSMA, and ET-1. Values show the mean mRNA levels relative to WT without stimulation (* p < 0.05). f Soluble collagen production from WT and ETBKO (n = 4 each) fibroblasts with or without BLM treatment (* p < 0.05). WT wild-type, αSMA α-smooth muscle actin, BLM bleomycin, Col1α1 collagen 1α1, ET-1 endothelin-1, ET B KO endothelin type B receptor knockout, PBS phosphate-buffered saline

BLM stimulation induced Col1α1 and ET-1 gene expression in fibroblasts from WT mice, but not in those from ETBKO mice. When stimulated with BLM, WT fibroblasts expressed the αSMA gene at significantly higher levels than did ETBKO fibroblasts (Fig. 5c-e).

ET-1 stimulation induced Col1α1 expression in WT fibroblasts. ET-1 also tended to induce αSMA mRNA in WT fibroblasts, although this increase did not reach statistical significance. ET-1 stimulation did not influence the Col1α1 or αSMA expression in ETBKO fibroblasts (Fig. 6a, b).
Fig. 6

Knockout of the ETB receptor signal reduces the activation of skin-derived fibroblasts in response to ET-1. a, b ET-1-induced fibroblast activation in WT and ETBKO mice (n = 4 or 5 each), determined by the gene expression levels of Col1α1, αSMA. Values show the mean mRNA levels relative to WT without stimulation (* p < 0.05). c Soluble collagen production from WT and ETBKO (n = 4 each) fibroblasts with or without ET-1-treatment (* p < 0.05). αSMA α-smooth muscle actin, BLM bleomycin, Col1α1 collagen 1α1, ET-1 endothelin-1, ET B KO endothelin type B receptor knockout, PBS phosphate-buffered saline, WT wild-type

Next, we measured soluble collagen content in the supernatant with Sircol collagen assay to assess whether BLM or ET-1 stimulation increases collagen production by fibroblasts. BLM or ET-1 treatment of WT fibroblasts significantly induced collagens. Increase in collagen production by BLM or ET-1 stimulation was not seen in ETBKO fibroblasts (Figs. 5f and 6c). Collectively, ETBKO fibroblasts showed less profibrotic properties in response to BLM or ET-1 than WT.

Discussion

In this study, we demonstrated for the first time with genetic ETBKO mice that ETB receptor signaling in the presence of the ETA receptor promotes fibrosis in BLM-induced scleroderma. Myofibroblast formation was inhibited in ETBKO mice, allowing them to resist BLM-induced skin fibrosis. At least one mechanism of the ETB receptor appears to function through dermal fibroblasts, because the ETBKO fibroblasts did not respond to BLM or ET-1 stimulation, whereas WT fibroblasts showed increased Col1α1 and αSMA expression in vitro.

Rescued ETBKO rats and mice, like those used in this study, are useful for investigating ETB receptor signaling. ETBKO rats show deteriorating health due to hypoxia-induced pulmonary hypertension, and ETBKO mice show worsened vascular remodeling in a carotid artery ligation model [27, 28]. Our study is the first to demonstrate that the ETB receptor is critical for BLM-induced scleroderma using ETBKO mice.

ET-1 is important in fibrosis because it induces collagen production and myofibroblasts. We found that in WT fibroblasts, BLM induced ET-1, which in turn induced collagen production. On the other hand, ETBKO fibroblasts did not produce collagen when stimulated by ET-1, indicating that ETB is indispensable for the ET-1-induced collagen production. Thus, the ET-1–ETB system is critical for the collagen production by fibroblasts.

We showed that myofibroblast formation was strongly inhibited in the ETBKO mice in vivo. In addition, ETBKO fibroblasts did not express αSMA mRNA in response to BLM or ET-1. These results indicate that ETB is involved in myofibroblast formation. In our experiments, ET-1’s induction of αSMA in WT fibroblasts in vivo was stronger than that in vitro. This was not surprising, because there are multiple sources of myofibroblasts in vivo, including tissue-resident fibroblasts [29], epithelial or endothelial cells transitioning into mesenchymal cells (EMT or EndoMT) [3033], or bone marrow-derived circulating fibrocytes [34, 35]. Thus, we believe that ETB is involved in myofibroblast formation from various types of cells.

Myofibroblast precursors differ in various tissues. For example, resident fibroblasts are the main contributors to myofibroblasts in lung fibrosis [36], and hepatic stellate cells are the most important source of myofibroblasts in liver fibrosis [37]. Although a recent study found that adipocytes differentiate into myofibroblasts in dermal fibrosis [38], the primary source of myofibroblasts in dermal fibrosis remains unclear. ETB receptor signaling seems to be important in liver and cardiac fibrosis [3941], but not renal fibrosis [42]. The difference of the skin and lung fibrosis might come from the difference in both myofibroblast precursor and contribution of ETB receptor signaling in the organ. Further investigation is needed to reveal which cells are responsible for generating dermal myofibroblasts, and how the ETA and ETB receptors are involved in dermal or other organ fibrogenesis.

In dermal fibroblasts, both ETA and ETB receptor signaling are reported to be necessary for ET-1 to exert its profibrotic effect [12]; in that study, neither ETA nor ETB receptor selective antagonists inhibited the collagen synthesis in dermal fibroblasts stimulated with ET-1. Our data appear to conflict with that study; this discrepancy might be due to differences between a pharmacological blockade and genetic knockout. The genetic knockout is assumed to affect permanently and completely, while the effect of pharmacological blockade is usually temporary and depends on affinity. We did not perform in vivo and in vitro study with the ETB selective antagonist, because it was reported that existing inhibitors could not suppress the fibroblast activation in vitro as mentioned above. We hope that new ETB selective antagonists that suppress fibroblast function will be developed.

Clinically, dual ETA/ETB receptor antagonists (bosentan, macitentan) and a selective ETA receptor antagonist (ambrisentan) improve the hemodynamics, exercise capacity, and survival rate in patients with pulmonary arterial hypertension [911]. These ET receptor blockers are also effective for preventing and improving digital ulcers in SSc patients [43, 44]. Currently, there is no selective ETB receptor antagonist that can be safely administered to humans. However, our study suggests that ETB receptor blockade is a potential pharmaceutical treatment for progressive skin fibrosis in SSc patients.

Conclusions

This study described that ETBKO mice were resistant to BLM-induced skin sclerosis and that ETBKO mice showed less fibroblast activation and myofibroblast formation in response to BLM or ET-1. Thus, ET-1–ETB receptor signaling is involved in skin sclerosis and in collagen synthesis by dermal fibroblasts.

Abbreviations

αSMA: 

alpha-smooth muscle actin

BALF: 

bronchoalveolar fluid lavage

BLM: 

bleomycin

BSA: 

bovine serum albumin

cDNA: 

complementary DNA

Col1α1: 

collagen 1α1

DMEM: 

Dulbecco's modified Eagle's medium

DβH: 

human dopamine β-hydroxylase

EDNRA: 

endothelin receptor type A

EDNRB: 

endothelin receptor type B

ET-1: 

endothelin-1

ETA

endothelin type A

ETB

endothelin type B

ETBKO: 

endothelin type B receptor-knockout

FBS: 

fetal bovine serum

GAPDH: 

glyceraldahyde-3-phosphate dehydrogenase

PBS: 

phosphate-buffered saline

PCR: 

polymerase chain reaction

SEM: 

standard error of the mean

SSc: 

systemic sclerosis

WT: 

wild-type

Declarations

Acknowledgements

The authors thank Shino Tanaka for providing technical assistance.

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Authors’ Affiliations

(1)
Department of Rheumatology and Clinical Immunology, Kobe University Graduate School of Medicine
(2)
Department of Clinical Pharmacy, Kobe Pharmaceutical University
(3)
Division of Cardiovascular Medicine, Department of Internal Medicine, Kobe University Graduate School of Medicine
(4)
International Institute for Integrative Sleep Medicine (WPI-IIIS), University of Tsukuba

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