Adenosine A2A receptors promote collagen production by a Fli1- and CTGF-mediated mechanism
© Chan et al.; licensee BioMed Central Ltd. 2013
Received: 30 July 2012
Accepted: 11 May 2013
Published: 11 May 2013
Adenosine, acting through the A2A receptor, promotes tissue matrix production in the skin and the liver and induces the development of dermal fibrosis and cirrhosis in murine models. Since expression of A2A receptors is increased in scleroderma fibroblasts, we examined the mechanisms by which the A2A receptor produces its fibrogenic effects.
The effects of A2A receptor ligation on the expression of the transcription factor, Fli1, a constitutive repressor for the synthesis of matrix proteins, such as collagen, is studied in dermal fibroblasts. Fli1 is also known to repress the transcription of CTGF/CCN2, and the effects of A2A receptor stimulation on CTGF and TGF-β1 expression are also examined.
A2A receptor occupancy suppresses the expression of Fli1 by dermal fibroblasts. A2A receptor activation induces the secretion of CTGF by dermal fibroblasts, and neutralization of CTGF abrogates the A2A receptor-mediated enhancement of collagen type I production. A2AR activation, however, resulted in a decrease in TGF-β1 protein release.
Our results suggest that Fli1 and CTGF are important mediators of the fibrogenic actions of adenosine and the use of small molecules such as adenosine A2A receptor antagonists may be useful in the therapy of dermal fibrosis in diseases such as scleroderma.
KeywordsFibrosis fibroblast scleroderma
Matrix production is critical for wound healing and tissue repair but in some clinical settings overproduction of matrix provides the basis for organ injury and dysfunction . In previous studies, we have demonstrated that occupancy of adenosine A2A receptors by an appropriate agonist, such as CGS-21680, promotes more rapid wound closure in both normal mice and diabetic rats and the enhancement in dermal wound healing is accompanied by an increase in matrix (collagen) in the wounds [2–4]. We have recently shown that pharmacological A2AR blockade can be used to diminish scarring while improving the collagen composition and tensile strength of the healed wound . Adenosine A2A receptor agonists such as CGS21680 do not promote wound healing in mice lacking adenosine A2A receptors and these same A2A receptor-deficient mice are protected from the development of hepatic and dermal fibrosis as well [6, 7]. Although exogenous adenosine receptor agonists may promote wound healing, endogenous adenosine production also contributes to wound healing and pathologic fibrosis because mice lacking adenosine A2A receptors have prolonged wound healing and mice that underproduce adenosine in response to appropriate stimuli due to deletion of ecto-5'nucleotidase are protected from the development of hepatic fibrosis [4, 8]. Consistent with the role of matrix overproduction in organ fibrosis and dysfunction, we have further demonstrated that adenosine and its receptor play a critical role in models of hepatic fibrosis/cirrhosis and dermal fibrosis in a model of scleroderma [6, 7, 9] and others have reported that adenosine plays a role in postoperative abdominal adhesions .
Although adenosine and adenosine A2A receptors regulate the function of many cell types that stimulate matrix production and fibrosis indirectly, we have reported that stimulation of the A2A receptor on matrix producing fibroblasts in the skin and stellate cells in the liver directly stimulates collagen production [6, 7]. In a murine model deficient for adenosine deaminase, a key catabolizing enzyme for adenosine, we have shown that fibrosis developed spontaneously in the skin in the absence of exogenous fibrogenic stimulators, concomitant with an increase in adenosine levels in the skin . In primary human dermal fibroblasts, the collagen-inducing effect of adenosine can be attributed directly to A2A receptor occupancy, since it is not attenuated by A1 receptor or A2B receptor antagonism, and A3 receptors are not expressed on human dermal fibroblasts . Furthermore, A2A receptor-deficient mice or mice treated with an A2A receptor antagonist are protected against induction of fibrogenesis in the skin by administration of bleomycin . A2A receptor antagonism also diminished dermal fibrogenesis in adenosine deaminase-deficient mice . Lazzerini et al. have shown that expression of adenosine A2A receptors are increased three-fold in dermal fibroblasts isolated from scleroderma patients compared to non-diseased controls, and A2A receptor ligation promotes collagen synthesis in dermal fibroblasts . The adenosine A2A receptor is a GS-linked receptor that stimulates cAMP accumulation and other downstream signals that mediate activation of collagen production by fibroblasts and stellate cells. A number of downstream signals play a role in the stimulation of collagen production by stellate cells including activation of the downstream kinases ERK1/2 (linked to collagen type I production) and p38 MAPKinase (linked to collagen type III production) .
Matrix production depends on the balance between forces that promote the transcription of matrix-producing genes and those that repress them. One of the best characterized of such repressors to date is friend leukemia integration-1 (Fli1), a member of the E26 transformation-specific (Ets) transcription factor family [13–16]. Reduction of Fli1 levels in dermal fibroblasts is associated with increased synthesis of connective tissue growth factor (CTGF/CCN2) and type I collagen, as well as a reduction of MMP-1 production [15–19]. This bears much similarity to the well known profibrotic effects of TGF-β. Indeed, enforced expression of Fli1 almost entirely abrogated TGF-β-induced profibrotic gene expression , suggesting that Fli1 is a potent endogenous antagonist of TGF-β signaling. Asano and colleagues have recently shown that TGF-β elicits PCAF-dependent acetylation of Fli1, which in turn results in its dissociation from the collagen promoter and subsequent degradation [20, 21]. We therefore hypothesized that one of the possible mechanisms for the fibrogenic effects of adenosine is mediated through suppression of Fli1 expression. Furthermore, since CTGF is a matrix-promoting growth factor regulated by Fli1 and is vastly overexpressed in adenosine deaminase-deficient mice [9, 19], it may also be an important regulator of A2A receptor-mediated fibrous tissue production.
Materials and methods
CGS-21680 was purchased from Sigma (St. Louis, MO, USA) and ZM-241385 was from Tocris (Ballwin, MO, USA). Antibody for human Fli1 was from BD Biosciences (San Jose, CA, USA), anti-CTGF and anti β-actin were from Santa Cruz Biotechnology (Santa Cruz, CA, USA), anti-human p84 was from Abcam (Cambridge, MA, USA) and anti-collagen I was purchased from Southern Biotech (Birmingham, AL, USA). Anti-mouse and anti-rabbit immunoglobulins were from DAKO (Carpinteria, CA, USA). DMEM and cell culture reagents were from Invitrogen (Grand Island, NY, USA).
Primary adult human dermal fibroblasts were purchased from Cambrex (East Rutherford, NJ, USA), or Lonza, Inc. (Allendale, NJ, USA). Fibroblasts were cultured in DMEM and used for experiments from first to the fifth passages. For CTGF neutralization, the human dermal fibroblasts where harvested during 16 hours and then incubated with the CTGF antibody (1:250) or normal serum as a control.
To examine expression of Fli1 protein, nuclear extracts from treated dermal fibroblasts were prepared following manufacturer´s instructions (Active Motif Nuclear Extract Protocol, Panomics, Fremont, CA, USA). Protein concentration was measured by BCA method (Pierce, Rockford, IL, USA) using bovine serum albumin as standard. Nuclear extracts (30 µg/lane) were electrophoresed in 12.5% SDS-polyacrylamide gel and transferred onto a nitrocellulose membrane (Bio-Rad, Hercules, CA, USA). The nitrocellulose membrane was blocked for two hours at room temperature in blocking solution (3% non-fat dry powdered milk in 1x Tween 20 Tris buffered saline (TTBS consisting of 20 mM Tris-HCl, pH 7.4, 150 mM NaCl and 0.1% Tween 20). After blocking, the membrane was incubated with primary antibody Fli1 (1:500; BD Pharmagen, San Jose, CA, USA), p84 (1:1,000; Abcam, Cambridge, MA, USA) or β-Actin (1:1,000; Santa Cruz Biotechnology Inc.,) overnight at 4ºC with gentle shaking on a platform shaker. After incubation with secondary antibody (rabbit anti-mouse immunoglobulins, 1:1,000 dilution, one hour, room temperature), proteins were visualized using the ECF kit (Amersham Biosciences, Little Chalfont, Buckinghamshire, UK). Band intensities were quantified by Adobe Photoshop 7.0.1 software and normalized to p84 nuclear marker level. To examine the expression of CTGF/CCN2, cells were plated 5x104/cm² into six-well plates, starved overnight when cell number reached 75% confluence and supernates were collected following treatment. Samples were concentrated using Microcon Ultracel YM-35 (Millipore, Billerica, MA, USA), and concentrated supernates were electrophoresed in a 10% SDS-polyacrylamide gel. CTGF/CCN2 was detected with primary anti-CTGF/CCN2antibody (1:1,000, Santa Cruz Biotechnology). Collagen type I was assessed in cell lysates as previously described .
Reverse transcription and Real-time PCR
Total RNA from treated primary human dermal fibroblasts was isolated using Trizol (Invitrogen, Carlsbad, CA, USA) following stimulation with CGS-21680 (10 µM) according to the manufacturer's protocol. RNA was quantified using spectrophotometric OD260 measurements and quality was assessed by OD260/ OD280 ratio. Reverse transcription was performed using the GeneAmp RNA Core Kit (Applied Biosystems, Carlsbad, CA, USA) in a volume of 25 µl using oligo dT primers and MuLV reverse transcriptase according to the manufacturer's protocol. Real-time PCRs were performed using the SYBR Green PCR Master Mix (Stratagene, Santa Clara, CA, USA) following the manufacturer's instructions and carried out on the Mx3005P™Q-PCR system (Stratagene). Aliquots of reverse transcription reactions were subjected to PCR in 25 µl reactions with SYBR® green using primers for Fli1 [5'- caacacggaagtgctgttgt-3' (forward), 5'-ccaaggggaggacttttgtt-3' (reverse)], CTGF/CCN2 [5'-ttccagagcagctgcaagta-3' (forward), 5'-ctcgtcacacacccactcc-3' (reverse), GAPDH [5'-accatcatccctgcctctac-3' (forward) and 5'-cctgttgctgtagccaaat-3' (reverse)], COL1A1 [5'-tgttcagctttggacctccg-3'(forward), 5'-ccgttctgtacgcaggtgattg-3' (reverse)], and COL3A1 [5'-gaagatgtccttgatgtgc-3'(forward), 5'-agccttgcgtgttcgatat-3'(reverse)].
Primers were designed using output Primer 3 software . The thermal cycling conditions included an initial 95°C for 300 s; then 95°C for 60 s, 58°C for 45 s and 72°C for 45 s for 40 cycles for Fli-1 and 95°C for 300 s; then 95°C for 60 s, 57°C for 45 s and 72°C for 45 s for 40 cycles for CTGF/CCN2. For each assay, standards, no-template and no-RT controls were included to verify the quality and cDNA specificity of the primers. Comparison of the expression of each gene between its control and stimulated states was determined with the delta-delta (ΔΔ)Ct, according to the following formula: (ΔΔ)Ct = ((CtGOI Control - Ct HKG Control) - (CtGOI Stim - Ct HKG Stim)), where GOI (gene of interest) corresponds to Fli1, CTGF or COL1A1 and HKG (housekeeping gene) corresponds to GAPDH. Fold increase was calculated according to the formula: Fold = 2 (ΔΔ)Ct .
Determination of transforming growth factor -β1
Normal human dermal fibroblasts were serum starved for 24 h and stimulated with CGS-21680 (1µM). Then, transforming growth factor β1 (TGF-β1) was determined in the supernates after removing the debris by centrifugation with the TGF-β1 ELISA kit (R&D Systems, Minneapolis, MN, USA) according to the manufacturer's protocol.
Results are represented as mean ± SEM. Data were analyzed by one-way ANOVA and significance of differences between groups was determined by Newman-Keuls method. Pairwise comparisons were made with the unpaired t-test. All statistical analyses were performed with Graphpad Prism software v. 4.02 (Graphpad Software, La Jolla, CA, USA).
Adenosine A2A receptor activation suppresses Fli1 expression in human dermal fibroblasts
Adenosine A2A receptor activation promotes CTGF secretion by dermal fibroblasts
CTGF is necessary for A2A receptor-mediated collagen type I production
A2AR activation prevents TGF-β1 release
We have previously shown that adenosine promotes fibrogenesis in the skin in vivo , that A2AR blockade prevents scarring in vivo  and activation of the adenosine A2A receptor but not A1 or A2B receptors promotes dermal extracellular matrix protein production including type I collagen in primary human dermal fibroblasts, and in a murine model of scleroderma . Others have shown that adenosine A2A receptor ligation increases collagen production and induces a pro-fibrotic phenotype in dermal fibroblasts isolated from scleroderma patients, in part by activation of the CB1 cannabinoid receptor .The present study strongly suggests, for the first time to our knowledge that an important mechanism for the adenosine-mediated promotion of fibrogenesis occurs at least in part through the regulation of the Ets factor, Fli1, and connective tissue growth factor (CTGF; CCN2). The importance of Fli1 in the regulatory mechanism involved in the transcriptional control of collagen gene expression has been well-described. Characterization of the COL1A2 promoter has identified a critical Ets-binding site mediating Fli1 inhibition . In fact, Fli1 has been previously described to function as a key regulator of the collagen homeostasis in the skin in vivo by repressing the collagen genes COL1A1, COL1A2, COL3A1, COL5A1 and COL5A2  and has also been shown to be significantly reduced in clinically involved skin of patients with scleroderma . Other studies have shown that inhibition of Fli1 by TGF-β and the subsequent displacement of Fli1 from the CTGF promoter results in the up-regulation of CTGF and the COL1A1 and COL1A2 genes in human dermal fibroblasts, strongly suggesting that TGF-β-mediated Fli1 suppression is involved in the activation of the profibrogenic gene program in fibroblasts . In this regard, the secreted protein CTGF [29, 30] is a major mediator of the profibrotic effects of TGF-β  and an important mediator of fibrosis since its constitutive expression in fibroblasts is sufficient to promote fibrotic disease in vivo .
Transforming growth factor (TGF-β) is known to be a critical regulator of matrix synthesis [26–28], and Fli1 is phosphorylated and acetylated following TGF-β1 treatment in dermal fibroblasts [21, 26–28]. On the other hand, acetylation of Fli1 by TGF-β1 renders the Fli1 protein less stable, providing an important mechanism for the pro-fibrotic actions of TGF-β1 [20, 26–28]. Previous reports suggest a link between dysregulation of Fli1 protein and scleroderma. Fli1 protein is markedly down-regulated in lesional fibroblasts from scleroderma patients . Epigenetic mechanisms may also be responsible, in part, for the repression of Fli1 gene in scleroderma in vivo and increased methylation of the Fli1 promoter region has been demonstrated in SSc fibroblasts and skin biopsies from SSc patients . Our prior work indicates that adenosine and the A2A receptor play a role in fibrosis in models of scleroderma. Mice lacking the A2A receptor are protected from development of dermal fibrosis following bleomycin exposure and A2A receptor activation promotes collagen type I and III production . We, therefore, sought to analyze if the A2A receptor regulates collagen production via Fli1 and CTGF pathways.
Our present studies have shown that adenosine A2A receptor activation in human dermal fibroblasts with the agonist CGS-21680 promotes a reduction of Fli1 mRNA and protein expression in the nucleus, as well as increases in CTGF mRNA and protein expression and secretion. These findings are consistent with previous observations that Fli1 directly inhibits CTGF expression, and knockdown of Fli1 dramatically up-regulates CTGF in dermal fibroblasts . Furthermore A2A receptor activation promotes an increase in collagen type I production which is prevented by CTGF neutralization (Figure 4B). This strongly suggests that Fli1 down-regulation and CTGF up-regulation precede collagen induction upon A2AR activation. Interestingly, release of TGF-β1 was reduced by A2AR activation. Our results therefore raise the possibility that A2AR and TGF-β1 may prevent excessive fibrosis by compensating its redundant pro-fibrogenic effects.
Recently, it has been suggested that hypoxia promotes fibrogenesis [33, 34]. In particular, hypoxia up-regulates CTGF expression through activation of HIF-1α in dermal fibroblasts from scleroderma patients, and thereby contributes to the progression of skin fibrosis . In this respect, as a critical mediator during hypoxia, the actions of adenosine are potentiated by HIF, which has been shown to stimulate the production of extracellular adenosine [36, 37], and suppresses both adenosine uptake into the intracellular compartment and its intracellular metabolism [36, 38, 39] (reviewed in ). In fact, although HIF-1α has been shown to up-regulate A2BR during conditions of hypoxia  suggesting a role for the A2BR in tissue protection , the A2AR may likely contribute to the role of adenosine in ischemic settings [39, 42]. Therefore, further studies will be needed to fully understand the interplay between hypoxia, HIF-1α and adenosine in skin fibrosis.
In summary, the results of our present work confirm previous observations of the role of the adenosine A2A receptor in the pathogenesis of dermal fibrosis in conditions such as scleroderma by promoting the production of tissue matrix and profibrotic mediators. These studies suggest new mechanisms for the profibrogenic effects of the A2A receptor by suppressing Fli1 expression and increasing CTGF secretion. Such mechanisms may play a role in matrix production in other fibrosing diseases, such as cirrhosis, and these mechanistic targets may be further explored as potential anti-fibrotic therapies.
Adenosine A2A receptor
collagen type I
Friend leukemia integration 1 transcription factor
connective tissue growth factor. HIF: Hypoxia-Inducible Factor.
This study was funded by grants from the National Institutes of Health AR057544 (EC), AR56672 and AR54897, (BC), AR42334 (MT), the Scleroderma Foundation (EC). In addition this work was supported by the NYU-HHC CTSI (UL1RR029893). The authors thank EUSTAR (EULAR Scleroderma Trials and Research Group), in particular, Dr. Oliver Distler, Dr. Tatiana Nevskaja and Prof. Marco Matucci-Cerinic for their help and participation in these studies.
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