Fibrosis accompanies most heart diseases and is associated with adverse patient outcomes. Transforming growth factor (TGF)β drives extracellular matrix remodelling and fibrosis in the failing heart. Some members of the ADAMTSL (a disintegrin-like and metalloproteinase domain with thrombospondin type 1 motifs-like) family of secreted glycoproteins bind to matrix microfibrils, and although their function in the heart remains largely unknown, they are suggested to regulate TGFβ activity. The aims of this study were to determine ADAMTSL2 levels in failing hearts, and to elucidate the role of ADAMTSL2 in fibrosis using cultured human cardiac fibroblasts (CFBs). Cardiac ADAMTSL2 mRNA was robustly increased in human and experimental heart failure, and mainly expressed by fibroblasts. Over-expression and treatment with extracellular ADAMTSL2 in human CFBs led to reduced TGFβ production and signalling. Increased ADAMTSL2 attenuated myofibroblast differentiation, with reduced expression of the signature molecules α-smooth muscle actin and osteopontin. Finally, ADAMTSL2 mitigated the pro-fibrotic CFB phenotypes, proliferation, migration and contractility. In conclusion, the extracellular matrix-localized glycoprotein ADAMTSL2 was upregulated in fibrotic and failing hearts of patients and mice. We identified ADAMTSL2 as a negative regulator of TGFβ in human cardiac fibroblasts, inhibiting myofibroblast differentiation and pro-fibrotic properties.
Fibrosis is a hallmark feature of heart failure, a leading cause of morbidity and mortality worldwide, and the degree of cardiac fibrosis is a strong predictor of poor outcomes in patients1,2,3,4. Cardiac fibrosis results from dysregulated deposition of extracellular matrix (ECM) molecules by activated cardiac fibroblasts (CFBs), termed myofibroblasts, leading to tissue stiffening5,6,7. Transforming growth factor (TGF)β is a central signalling molecule in cardiac development and disease, and a major driver of cardiac myofibroblast differentiation and fibrosis8,9,10. Inactive TGFβ, bound to latent TGFβ binding proteins (LTBPs), is stored in the ECM as the large latent complex (LLC), tethered to microfibrils11,12. Release from the inactive complex is required for TGFβ activation and initiation the pro-fibrotic response10. Thus, identification of molecular players governing TGFβ signalling in the heart is essential to develop novel treatment strategies that can counteract cardiac fibrosis.
Members of the ADAMTSL (a disintegrin-like and metalloproteinase domain with thrombospondin type 1 motifs-like) family of secreted glycoproteins structurally resemble ADAMTS proteases, but lack enzymatic activity, as they do not have a protease domain13,14. Some ADAMTS proteases have important roles in the heart15,16,17, but little is known about the role of ADAMTSLs. Emerging data suggests that they can bind and regulate fibrillin microfibrils18,19,20, major ECM components that control TGFβ bioavailability. Recessive loss-of-function ADAMTSL2 mutations cause geleophysic dysplasia (GD), an inherited connective tissue disorder resulting in severe musculoskeletal, pulmonary, and cardiac anomalies, with increased TGFβ levels and activity observed in patient-derived skin fibroblasts21,22. In beagles, an ADAMTSL2 founder mutation causes Musladin-Lueke Syndrome with severe skin and intermuscular fibrosis23. Adamtsl2−/− mice fail to survive past birth, likely as a result of lung anomalies associated with bronchial fibrillin microfibril accumulation, and have cardiac developmental defects24. Collectively, these data suggest that ADAMTSL2 regulates ECM deposition and TGFβ signalling and may thus have an important role in cardiac fibrosis and heart failure.
In the present study, we investigated expression of ADAMTSLs in heart failure, and identified novel functions of ADAMTSL2 in CFBs. Specifically, we found that ADAMTSL2 was robustly up-regulated in clinical and experimental heart failure, and ADAMTSL2 was predominantly expressed by CFBs. In cultured foetal and adult human CFBs, ADAMTSL2 negatively regulated TGFβ signalling, and attenuated myofibroblast differentiation and pro-fibrotic properties of CFBs.
ADAMTSL1-5 and Papilin are up-regulated in hearts of mice with fibrosis and failure
To understand the role of ADAMTSL proteins in heart failure, we determined ADAMTSL gene expression in left ventricles (LV) of mice subjected to AB for two, four and 20 weeks. The resulting cardiac phenotypes were previously reported25, and in summary show concentric hypertrophic remodelling at two and four weeks post-AB, where the heart muscle is thickened, and end-stage dilated heart failure at 20 weeks, with thinning of the heart muscle, compared to sham-operated controls. Cardiac fibrosis (increased collagen expression and extracellular deposition) and increased TGFβ signalling was present at all three time-points, with increased α-smooth muscle actin (α-SMA) observed at two weeks25. We found that all members of the Adamtsl family were upregulated after AB, except Adamtsl6, which was unchanged. Adamtsl2 showed the highest up-regulation with a four–eightfold increase during hypertrophic remodelling, and an eightfold increase at end-stage cardiac dilatation (Fig. 1a), suggesting a potential role in fibrosis and heart failure. Thus, we focused our efforts on ADAMTSL2.
Immunoblotting for ADAMTSL2 in LV protein extracts was consistent with Adamtsl2 mRNA induction, showing a 2-3.5-fold increase in full-length protein at two, four and 20 weeks post-AB (Fig. 1b,c). In situ hybridization (ISH) in heart sections showed that Adamtsl2 mRNA expression was increased in the LV and left atrium (LA) after AB, compared to modest expression of Adamtsl2 in the sham-operated mice (Fig. 1d–f). Importantly, increased Adamtsl2 expression in AB mice was seen between cardiomyocytes (CM) in the LV wall (Fig. 1d), in regions of the LV endocardium (Fig. 1e, arrows) and the LA endocardium (Fig. 1f), suggesting an increase in ADAMTSL2 expression in cell types other than CMs across the heart.
ADAMTSL2 is mainly expressed by cardiac fibroblasts in the ventricular wall
As two of the dominant cell types in the ventricular wall, we investigated expression of the ADAMTSLs in primary cultures of isolated CMs and CFBs from neonatal rat hearts. The purity of the cultures was confirmed by the cardiomyocyte marker Troponin-I (Tnni3), the endothelial cell marker von Willebrand Factor (Vwf), and the fibroblast markers type I Collagen (Col1a2), Periostin (Postn), and α-SMA (Acta2) (Supplementary Fig. S1a–c). Adamtsl1-4 were mainly expressed by CFBs, with fivefold higher Adamtsl2 expression in CFBs compared to CMs, while Papln expression was higher in CMs (Fig. 1g). As endothelial cells were enriched in the CM cultures, our data suggest CFBs as the main cellular source of ADAMTSL2 in the ventricle. In line with this, data mined from published single-cell RNA sequencing studies26 showed that Adamtsl2 was specifically expressed by fibroblasts and stromal cells (fibroblast lineage) in the mouse heart (Fig. 1h). Combined, these results indicate that CFBs constitute the main source of ADAMTSL2 in the heart.
ADAMTSL2 over-expression inhibits TGFβ signalling in human cardiac fibroblasts
To determine the role of ADAMTSL2 in CFBs, gain-of-function in vitro studies were performed. We over-expressed ADAMTSL2 using replication-deficient adenovirus 5 containing ADAMTSL2 (L2) or vehicle control (Veh) in hfCFBs. Successful over-expression was confirmed by increased ADAMTSL2 mRNA (Fig. 2a) and increased full-length, glycosylated protein in the cell cytosol, ECM and medium (Fig. 2b). Loss-of-function studies were considered, but deemed unsuitable, as basal ADAMTSL2 expression was barely detectable in our cultured hfCFBs (Supplementary Fig. S2a-c), in line with negligible detection of ADAMTSL2 mRNA in cultured human dermal fibroblasts from deceased organ donors in the GTEx project (dbGaP Acession phs000424.v8.p2) (Supplementary Fig. S2d).
Effects of increased ADAMTSL2 levels were investigated in hfCFBs at two stages of ECM maturation i.e. cells were transduced at day one of a four-day protocol (immature ECM) or at day four of a seven-day protocol (mature ECM) (Supplementary Fig. S3a). Matrix proteins showed differential gene expression in the two protocols (Supplementary Fig. S3b-c), and importantly, greater ECM accumulation was evident at seven days (Supplementary Fig. S3d). More LLC was incorporated into the mature ECM (Supplementary Fig. S3e), and the cells became less proliferative at this stage (Supplementary Fig. S3f.). Myofibroblast differentiation occurred within the first four days in culture, as evident from the peak expression at four days (Supplementary Fig. S3g) but persisted through seven days (Supplementary Fig. S3d,g). TGFβ signalling was comparable in the two protocols (Supplementary Fig. S3h). Thus, the seven-day protocol was used to investigate the role of ADAMTSL2 in a mature ECM, while the four-day protocol was used to study its role in a developing, immature ECM.
First, we assessed whether increased ADAMTSL2 affected TGFβ signalling in CFBs. We found that mRNA levels of direct downstream targets of TGFβ signalling in the heart, connective tissue growth factor (CTGF) and periostin (POSTN)27,28, were reduced 30–50% in L2 cells in both culture protocols (Fig. 2c). Canonical TGFβ signalling is mediated mainly through phosphorylation of SMAD2/3 transcription factors, which translocate to the nucleus8, and we found that L2 decreased SMAD2 phosphorylation (pSMAD) 50–70% in the two protocols (Fig. 2d). Correspondingly, the pSMAD2/3 complex translocated to the nucleus in Veh, but less so in L2 cells (Fig. 2e). Thus, our data demonstrate that ADAMTSL2 caused reduced TGFβ signalling in CFBs.
Next, we addressed how ADAMTSL2 reduced TGFβ signalling. To assess whether ADAMTSL2 inhibited the active, free form of TGFβ directly, or its interaction with the TGFβ receptor (TGFBR), recombinant, active TGFβ1 was added to Veh and L2 cells. Although L2 cells had lower levels of pSMAD at baseline, we found that TGFβ treatment increased pSMAD in both Veh and L2 cells, with a higher pSMAD increase in L2 cells relative to respective baseline levels (Fig. 2f). This demonstrated that ADAMTSL2 did not inhibit active TGFβ signalling, and indicate that the effect of ADAMTSL2 on TGFβ is upstream of active, released TGFβ. Immunoblotting for the small latency complex (SLC), consisting of TGFβ bound to latency associated peptide (LAP), showed a 35% reduction of SLC in L2 cells (Fig. 2g), suggesting reduced TGFβ production. Furthermore, mRNA expression of TGFB1 was reduced to 85% of control in the immature ECM culture and TGFB3 to 60–75% of controls in the immature and mature ECM cultures (Fig. 2h). In line with reduced production of TGFβ, we found that LTBP1 and the LLC were reduced in L2 cell fractions from the cytosol, ECM, and medium of mature ECM hfCFB cultures. (Fig. 2i–j). There was no change in gene expression of the three LTBP isoforms that bind TGFβ, namely LTBP1, LTBP3 and LTBP4 (Supplementary Fig. S4a-c), indicating protein-level regulation. Finally, CFB treatment with recombinant TGFβ1 resulted in a 1.6-fold increase in ADAMTSL2 mRNA levels that was returned to baseline upon co-treatment with the TGFβ-SMAD inhibitor SB431542 (Fig. 2k). These results suggest that ADAMTSL2 is under transcriptional control of TGFβ signalling, and that ADAMTSL2 regulates TGFβ as part of a negative feedback loop.
ADAMTSL2 alters expression levels of ECM and ECM-associated genes in cardiac fibroblasts
We next examined whether ADAMTSL2 over-expression altered production of major ECM constituents. As the classical definition of cardiac fibrosis is the accumulation of fibrillar collagens5, we quantified the amount of newly synthesized collagen in immature ECM hfCFB cultures. However, we found no difference in collagen synthesis (Fig. 3a). Thus, despite inhibiting TGFβ signalling, ADAMTSL2 did not affect levels of structural collagens in cultured hfCFBs.
To address whether ADAMTSL2 regulated ECM microfibrils we measured the expression of fibrillin-1 (FBN1), fibrillin-2 (FBN2) and tropoelastin (ELN) in L2 cells. The mRNA level of FBN1 was reduced to 80% of control in the immature ECM culture, and ELN to 40–60% of controls in both cultures, while mRNA levels of FBN2 were increased 1.2-fold in both cultures (Fig. 3b,c). These results suggest that ADAMTSL2 may regulate the composition of tissue microfibrils in the cardiac ECM.
Using array expression analysis of 84 ECM and cell adhesion genes (see Supplementary Fig. S5), we found 50 differentially expressed genes ± 0.5-fold or more (31 down-regulated/19 up-regulated) in L2 cells (Fig. 3d). Proteins involved in cell adhesion, proliferation and spreading, such as integrin β3 (ITGB3), contactin-1 (CNTN1), E-cadherin (CDH1) and tenascin C (TNC) were down-regulated, while adhesion molecules related to inflammation, vascular cell adhesion molecule-1 (VCAM1), L-selectin (SELL) and P-selectin (SELP), were among the most up-regulated. Collagen degrading enzymes such as matrix metalloproteinase 1 and 13 (MMP1, MMP13), as well as non-fibrillar collagens (COL6A1, COL6A2, COL8A1, COL14A1, COL16A1) were also among the up-regulated. Strikingly, osteopontin mRNA (SPP1) was down-regulated to 6% of controls (Fig. 3d). As both TGFβ and osteopontin signalling are required myofibroblast differentiation8,29, this indicate that ADAMTSL2 inhibited myofibroblast differentiation.
ADAMTSL2 inhibits myofibroblast differentiation and regulates cardiac fibroblast function
We confirmed negative osteopontin regulation in L2 cells, and found that SPP1 was reduced to 5% and 30% of controls, in our immature and mature ECM hfCFB cultures, respectively (Fig. 4a). We next investigated myofibroblast markers and found that expression of ACTA2, encoding α-SMA, was reduced 50% in both culture protocols (Fig. 4b). Correspondingly, immunoblotting showed a 30–40% reduction of α-SMA protein (Fig. 4c), and a strong reduction in α-SMA immunostaining (Fig. 4d). These results indicate that ADAMTSL2 inhibits cardiac myofibroblast differentiation.
Upon further investigation of characteristic myofibroblast properties we found that increased ADAMTSL2 resulted in reduced vinculin mRNA and protein levels (Fig. 4e), reduced focal adhesion kinase (FAK) activation and phosphorylation of paxillin (Fig. 4f), and impaired stress fibre formation, illustrated by reduced phalloidin immunostaining (Fig. 4g). Levels of the cell proliferation markers proliferative cell nuclear antigen (PCNA), mini-chromosome maintenance protein 2 (MCM2) and marker of proliferation Ki-67 (KI67) were reduced to 50–80% of controls (Fig. 4h), indicating that ADAMTSL2 inhibits CFB proliferation. In line with this, incorporation of EdU during DNA synthesis was reduced in L2 cells, corresponding to reduced proliferation (Fig. 4i). A scratch assay was performed to assess cell migration, and L2 cells showed reduced migration across the gap compared to Veh (Fig. 4j). As the hallmark feature of myofibroblasts, we assessed whether ADAMTSL2 affected CFB contraction, and found that the ability to contract collagen gels was impaired in L2 cells (Fig. 4k).
To assess whether myofibroblast differentiation could be rescued by treatment with TGFβ, recombinant, active TGFβ1 was added to the Veh and L2 cultures. Protein expression of α-SMA increased in both conditions, relative to respective baseline levels, following treatment (Fig. 4l). This indicates that ADAMTSL2 may inhibit myofibroblast differentiation through inhibition of TGFβ. Collectively, these data show that ADAMTSL2 modulated CFBs towards a less myofibroblastic and less fibrotic phenotype.
Extracellular ADAMTSL2 inhibits TGFβ signalling in human cardiac fibroblasts
To determine whether the observed effects of ADAMTSL2 over-expression were due to ADAMTSL2’s function in the extracellular environment, hfCFBs were treated with conditioned medium from L2 cells (L2-medium), which had demonstrably higher levels of ADAMTSL2 (Fig. 5a), or controls (Veh-medium). In line with ADAMTSL2 over-expression, treatment with L2-medium resulted in reduced expression of TGFB1, CTGF, POSTN and ACTA2, but still unaltered LTBP1 expression, compared to Veh-medium (Fig. 5b). Furthermore, cells treated with L2-medium showed reduced phosphorylation of SMAD2 and reduced levels of α-SMA (Fig. 5c–d). To determine whether extracellular ADAMTSL2 would affect the active, free form of TGFβ, Veh- and L2-medium was pre-incubated with recombinant TGFβ and added to untreated hfCFBs. Both conditions resulted in similar increase in pSMAD after 30 and 60 min of treatment, confirming that ADAMTSL2 does not directly bind and inhibit free, active TGFβ (Fig. 5e). Thus, these data confirmed the findings from over-expression of ADAMTSL2, and showed that hfCFBs respond to increased extracellular ADAMTSL2 with reduced TGFβ activity and myofibroblast differentiation.
ADAMTSL2 is increased in human hearts with fibrosis and heart failure
Finally, from a translational perspective, we investigated ADAMTSL2 levels in hearts of patients with heart failure and assessed the effects of ADAMTSL2 in human adult CFBs (haCFBs). From the GTEx project of deceased organ donors, it was evident that ADAMTSL2 was expressed in human hearts, both in left ventricle and atrial appendage (Supplementary Fig. S2d and Table S3). We determined ADAMTSL2 mRNA levels in myocardial biopsies from three cohorts of patients, namely aortic stenosis (AS), hypertrophic obstructive cardiomyopathy (HOCM) and dilated cardiomyopathy (DCM) vs. respective controls. Patient characteristics were reported previously, with hypertrophic remodelling, fibrosis and heart failure with preserved ejection fraction (HFpEF) in AS and HOCM, and dilated heart failure with reduced ejection fraction (HFrEF) and fibrosis in DCM patients30,31,32. Importantly, ADAMTSL2 mRNA was increased 2.5-fold in LVs of HOCM, DCM and AS patients (Fig. 6a). Immunoblotting of LV extracts confirmed increased full-length ADAMTSL2 protein in biopsies from HOCM and DCM patients (Fig. 6b-c and Supplementary Fig. S6). Biopsies from the AS patients were exclusively used for mRNA analyses due to small sample size. Finally, ADAMTSL2 was successfully over-expressed in haCFBs in a four-day protocol similar to hfCFBs (see Supplementary Fig. S3), and we found that mRNA levels of CTGF, POSTN, ACTA2, SPP1 and PCNA were reduced compared to controls (Fig. 6d). Thus, the increased levels of Adamtsl2 observed in experimental heart failure was confirmed in human heart failure, and our findings from hfCFBs translated to ventricular haCFBs.
The present work places the ADAMTSL family of ECM glycoproteins on the map of influential molecules in the failing heart. We found that six out of seven Adamtsl proteins were up-regulated in hearts of mice with AB-induced heart failure and fibrosis. In particular, ADAMTSL2 mRNA and protein levels were robustly increased in both experimental and clinical heart failure. In the heart, Adamtsl2 was mainly expressed by CFBs, and increased levels of ADAMTSL2 in human CFBs in vitro, through viral over-expression or exposure to ADAMTSL2-containing conditioned medium, resulted in reduced TGFβ production and activity. Increased ADAMTSL2 levels inhibited myofibroblast differentiation, and attenuated important pro-fibrotic, phenotypic properties of CFBs i.e. proliferation, migration and contractility. Taken together, our data indicate that ADAMTSL2 is a negative regulator of TGFβ and the fibrotic response in CFBs.
A central finding in our study is that increased levels of extracellular ADAMTSL2 attenuated canonical TGFβ signalling in human CFBs, shown through reduced intracellular SMAD activation and nucleus translocation, and reduced expression of specific TGFβ target genes. This is in line with the increased TGFβ levels and activity observed in isolated dermal fibroblasts from patients with GD, caused by ADAMTSL2 loss-of-function mutations22, in HEK293 cells transfected with the GD-causing ADAMTSL2 mutation p.Gly296Arg33, and in chondrocytes isolated from Adamtsl2−/− mice34. Thus, our findings were consistent with the existing literature on non-cardiac cells, and we identified that increased ADAMTSL2 levels resulted in both reduced TGFβ amounts and activity in fibroblasts of the heart. As TGFβ signalling is central to cardiac fibrosis, this is a novel finding with possible implications for limiting fibrosis in heart failure.
TGFβ regulation is extremely complex, with positive and negative feedback loops, and its activity is largely regulated by extracellular activation35,36. We found that extracellular ADAMTSL2 did not inhibit the active, free form of TGFβ in the extracellular environment, indicating that the effect of ADAMTSL2 on TGFβ1 must be up-stream, or at the level of, TGFβ1 activation in the ECM. Previous studies have demonstrated that ADAMTSL2 binds directly to LTBP1 and fibrillin-1 and -222,24,37,38, potentially forming a complex in the ECM. Thus, we speculate that ADAMTSL2 might inhibit TGFβ through this interaction. Mechanistically, we suggest that increased extracellular ADAMTSL2 inhibits TGFβ complex deposition in the ECM, through direct binding of the LLC, or through competitive binding of fibrillin microfibrils, thus limiting the amount of TGFβ that is available for activation. Alternatively, ADAMTSL2 may stabilize the LLC on fibrillin microfibrils, preventing TGFβ release, however, this seems less likely as we found reduced levels of LLC in the ECM of L2 cells.
As TGFβ positively regulates its own gene expression35,39,40, less TGFβ activity may cause the observed reduction in TGFB1 expression and protein production in L2 cells. Treatment with active, recombinant TGFβ increased endogenous ADAMTSL2 expression in CFBs, indicating that ADAMTSL2 is part of a negative feedback loop, in which TGFβ increases its own inhibitor. Indeed, ADAMTSL2 expression was recently shown to be controlled by TGFβ during fibrous tissue differentiation in the sclerotome41, supporting this theory. However, the molecular mechanisms underlying the reduction in TGFβ production and activity by ADAMTSL2 remain to be elucidated.
Our analysis of multiple facets of CFB phenotype showed that ADAMTSL2 inhibited cardiac myofibroblast differentiation. This was seen through reduced α-SMA and osteopontin expression, signature molecules of the myofibroblast. Additionally, CFB characteristics shifted towards a less fibrotic phenotype, with reduced stress fibre formation, focal adhesion and migration, as well as reduced proliferation, in response to increased ADAMTSL2. The latter is in line with increased proliferation of Adamtsl2-deficient chondrocytes34. Importantly, the ultimate defining feature of the myofibroblast, contractility42, was inhibited by ADAMTSL2. Since expression of α-SMA and osteopontin is essential for development of cardiac fibrosis29, our results suggest that ADAMTSL2 reduces pro-fibrotic effects of CFBs. As addition of TGFβ rescued the expression of α-SMA, the effects of ADAMTSL2 on myofibroblast differentiation was likely mediated through TGFβ.
ADAMTSL2 mutations cause recessive GD (MIM #231,050) in humans, a severe connective tissue disorder with poor prognosis, in which cardiac anomalies, such as progressive valve thickening, are found20. In beagles, an Adamtsl2 loss-of-function founder mutation causes Musladin-Lueke Syndrome, with severe skin and intermuscular fibrosis23 and Adamtsl2-/- mice die shortly after birth due to bronchial occlusion with accumulated fibrillin microfibrils, in addition to cardiac malformations24. The phenotypic evidence from ADAMTSL2 mutations in humans, mice and dogs suggests that ADAMTSL2 could limit cardiac fibrosis, possibly through regulation of collagen and microfibrils24,34,37. We did not observe changes in collagen synthesis in our CFB cultures, but we found that ADAMTSL2 affected expression of core microfibril components: fibrillin-1, fibrillin-2 and tropoelastin, suggesting that ADAMTSL2 is modulating cardiac ECM composition. However, elastic fibres are difficult to study in culture, and in vivo studies would have to be performed to settle the role of ADAMTSL2 in regulation of microfibrils in the heart.
In the failing heart, adaptive brakes are expressed to counteract the maladaptive drivers. A prime example of an adaptive brake is the hallmark heart failure blood and tissue biomarker brain natriuretic peptide (BNP), which was recently included in the treatment guidelines1,43. We speculate that elevated levels of ADAMTSL2 in patients and mice with fibrosis and heart failure could be beneficial, similar to BNP. The lack of experiments examining the in vivo role of ADAMTSL2 in cardiac remodelling, fibrosis and failure is therefore a significant limitation of our study. Such experiments are complicated by the fact that Adamtsl2−/− mice are non-viable24. Nevertheless, heterozygous Adamtsl2−/+ mice, or mice with global post-natal or fibroblast-specific conditional Adamtsl2 inactivation could be utilized. Efforts to increase ADAMTSL2 experimentally during heart failure progression, e.g. with an AAV vector, should also be made to evaluate the effects of ADAMTSL2 in vivo. Thus, whether increased cardiac ADAMTSL2 has beneficial effects in the diseased heart remains to be elucidated in future experiments.
In conclusion, the extracellular matrix-localized glycoprotein ADAMTSL2 was upregulated in fibrotic and failing hearts of patients and mice. ADAMTSL2 inhibited TGFβ and myofibroblast differentiation, reduced the expression of pro-fibrotic signature molecules and attenuated central pro-fibrotic properties of human CFBs. Mechanistically, we showed that ADAMTSL2 over-expressing cells produce less TGFβ, and speculate that ADAMTSL2 inhibits TGFβ deposition and activation, contributing to a negative TGFβ feedback loop. We suggest that ADAMTSL2 may have anti-fibrotic effects in the failing heart.
An expanded Supplementary Methods section is available in the Supplementary Information.
The human cardiac biopsy protocol was approved by the Regional Committee for Medical Research Ethics (REK IDs 07482a, S-02292/2017–570 and 2010/2226), the South-Eastern Regional Health Authority of Norway, and was in accordance with the Declaration of Helsinki. Informed consent was signed by all patients and the next of kin of heart donors. Mouse protocols were approved by the Norwegian National Animal Research Committee (approval 8041), and conformed to the NIH Guide for the Care and Use of Laboratory Animals (NIH publication no. 85-23, revised 2011) and the ARRIVE guidelines for reporting of animal research44.
Human heart tissue samples
Left ventricular (LV) tissue biopsies were obtained at Oslo University Hospital, Norway, from patients with heart disease of three aetiologies, Aortic stenosis (AS, n = 11), hypertrophic obstructive cardiomyopathy (HOCM, n = 15) and dilated cardiomyopathy (DCM, n = 20). All patients received standard clinical evaluation, treatment and follow-up in accordance with Oslo University Hospital guidelines. Patient characteristics have been previously described30,31,32. For detailed method description, see Supplementary Methods 3.1.
Mouse pressure overload heart failure model
Mouse heart samples used for this study were derived from a previously published cohort25. In brief, experimental heart failure was induced in 8–10 week-old C57BL/6 J mice by aortic banding (AB) of the ascending aorta, causing pressure overload of the LV. Hearts were harvested at two, four and 20 weeks post-AB. Analgesia was administered pre- and post-operatively by subcutaneous injection of (0.3 mg/mL) buprenorphine, with additional analgesics given based on the status of the animal. The mice were euthanized by dissection of the heart under deep terminal anaesthesia breathing 3% isoflurane. For detailed method description, see Supplementary Methods 3.2.
In-situ hybridization of mouse heart sections
In situ hybridization was performed on sectioned, paraffin-embedded, AB- or sham-operated mouse hearts using an RNAscope technology with a probe specific for mouse Adamtsl2. Hematoxylin was used as the counterstain. For full method description, see Supplementary Methods 3.3.
Cultures of neonatal rat cardiac myocytes and fibroblasts
Primary cultures were prepared as described previously45. Briefly, CMs and CFBs were isolated from hearts of 1–3 day old neonatal rats (Wistar). Cells were plated at 3.8 × 104 cells/cm2cultured in serum-containing Dulbecco’s Modified Eagle medium in a 37 °C, 5% CO2 humidified incubator. The purity of the cultures was determined by expression analysis of the CM-specific gene Tnni3, the endothelial cell marker Vwf, and the fibroblast markers Col1a2, Postn, and Acta2 (see Supplementary Fig. S1a-c). For full method description, see Supplementary Methods 3.4.
Human cardiac fibroblast cultures
Commercially available human foetal (Cell Applications) and adult (PromoCell) cardiac fibroblasts (hfCFBs and haCFBs, respectively) were used for cell culture experiments with the recommended culture media. In summary, cells were plated at 20,000 cells/cm2 and cultured for four days (generating an immature, developing ECM) or 10,000 cells/cm2 and cultured for seven days (generating a mature ECM) before harvest (see Supplementary Fig. S3). Cells were kept at 37˚C, in a 5% CO2 humidified incubator. Adenoviral transduction for over-expression of ADAMTSL2 (L2) or vehicle control (Veh) was performed one or four days after seeding in cultures with immature or mature ECM, respectively. Transduction was performed in serum-containing medium for 24 h, followed by serum-free medium for 48 h. Non-transduced cells were treated with conditioned medium, containing ADAMTSL2 protein (L2-medium), or control (Veh-medium) diluted 1:1 in serum-free medium, for three days. Cells were harvested 72 h after seeding. Transduced cells were treated with recombinant TGFβ (10 µg/µL) for 24 h following 24 h serum starvation. Non-transduced cells were treated with recombinant TGFβ (10 µg/µL) and/or TGFβ-SMAD inhibitor (10 µM) for 2 h following 24 h serum starvation. Non-transduced cells were treated with L2 or Veh conditioned medium, pre-incubated for 1 h with recombinant TGFβ1 (10 µg/µL), for 0, 30 and 60 min before harvest. For detailed method description, see Supplementary Methods 3.5.
hfCFBs were cultured on coverslips, fixed in 4% PFA, permeabilized and incubated with primary antibodies for α-SMA, fibrillin-1, EDA-fibronectin, LTBP1 and Collagen type I, and fluorescently labelled secondary antibodies. Cells were mounted onto slides and proteins were visualized with the Axioscan Z1 (Carl Zeiss) for full slide scanning, or the LSM 710 confocal microscope (Zeiss). For full method description, see Supplementary Methods 3.6.
Collagen gel contraction assay
hfCFBs transduced with Veh or L2 were mixed with collagen and added to BSA-coated plates. The gels were allowed to polymerize before serum-free medium was added to release the gels from the surface. Contraction was observed over the next 24 h, percent contraction was calculated by measuring the circumference of the collagen gels. For full method description, see Supplementary Methods 3.7.
EdU incorporation assay
hfCFBs transduced with Veh or L2 were seeded in serum-containing medium at 103 cells/cm2 in 96-well plates. After 24 h, serum-free medium, or serum-containing medium for positive control, was added. After 48 h, cells were labelled with EdU (10 µM) for 2 h. Cells were fixed according to protocol (Click-iT™ EdU Proliferation Assay, Cat# C10499, CyQUANT, Invitrogen) and fluorescence was measured on the Hidex microplate reader.
Cell monolayer scratch migration assay
hfCFBs were seeded and transduced in 12-well plates, and kept in serum-free medium for 24 h. A 1 mm wide scratch was made through the cell monolayer using a 200 µL pipette tip and fresh serum-free medium was added. Cell migration across the gap was observed and images were taken with the Eclipse Ts100 phase contrast microscope. Percent migration was calculated from the size of the scratch at 24 h using ImageJ (NIH).
[3H] proline incorporation assay
hfCFBs were seeded and transduced in 12-well plates. After 24 h, serum-free medium containing ascorbic acid (50 µM/mL) and L-[2,3-3H]-Proline (1 µCi, Cat# NET323001MC, Perkin Elmer) was added. After 48 h, cells were lysed in NaOH (1 M) and diluted in OptiPhase HiSafe 3 liquid scintillation cocktail (Cat# 1200.437, Perkin Elmer). Amount of incorporated radiolabelled proline, a surrogate for collagen biosynthesis46, was measured on the Wallac Winspectral 1414 liquid scintillation counter (Perkin Elmer).
Gene expression analysis
Total RNA was isolated from LVs and cell cultures, and relative gene expression was determined using TaqMan probes (Supplementary Table S1) or TaqMan array plates. Gene expression was normalised to housekeeping genes 60S ribosomal protein L32 (RPL32), L4 (RPL4), or glyceraldehyde 3-phosphate dehydrogenase (GAPDH). For full method description, see Supplementary Methods 3.8.
Gene expression data mined from available online databases
The Single Cell Expression Atlas database (https://www.ebi.ac.uk/gxa/sc/home, EMBL-EBI, Cambridgeshire, UK, accessed on 11.07.2021) was used to mine for published single cell RNA sequencing data describing Adamtsl2 expression in different organs and cell types. The Genotype-Tissue Expression (GTEx) Project Portal (https://gtexportal.org/home/, Broad Institute, Boston, MA, accessed on 11.07.2021) was used to analyse ADAMTSL family expression (RNA sequencing) in cultured dermal fibroblasts, atrial appendage and left ventricle of deceased organ donors. Charts were created using the interactive graphics functionality of the databases.
Protein isolation and immunoblotting
Protein lysates from mouse and human LVs were extracted as previously described25,45, using a PBS‐based lysis buffer containing 1% Triton X‐100. Protein lysates from cell cultures were extracted using the buffer above, or a buffer containing 1% SDS for retrieval of ECM proteins. For studying LTBP1 in cytosolic and ECM protein fractions, cells were lysed using a NP-40-based lysis buffer and fractioned through centrifugation. For studying nuclear translocation of pSMAD, cells were lysed and proteins fractioned using the compartment protein extraction kit (Merck Millipore) according to the manufacturer’s protocol. Secreted proteins were harvested from the cell culture medium. Supernatants and lysates were stored at − 20 °C. N-linked oligosaccharides were enzymatically removed from glycosylated proteins using PNGaseF. Western blotting was performed using the Trans-Blot Turbo blotting system (Bio-Rad). Membranes were blocked in 5% non-fat dry milk, casein or BSA, before incubation with primary antibodies (see Supplementary Table S2) and species-specific horseradish peroxidase secondary antibodies. For full method description, see Supplementary Methods 3.9.
Data are expressed as the minimum value, group mean, and maximum value, with all data points shown in graphs, relative to respective controls and to a reference gene/protein. Normal data distribution was evaluated using the Shapiro–Wilk test. Statistical differences were tested in GraphPad Prism 8, using the unpaired Student t-test when comparing two groups, the one-way ANOVA with Tukey’s multiple comparisons test when comparing multiple groups, and the two-way repeated measures ANOVA with the Geisser-Greenhouse correction when comparing multiple time-points. P-values < 0.05 were considered statistically significant, and exact p-values are given in the figures, unless P < 0.001.
All data generated or analysed during this study are included in this published article and its Supplementary Information.
Alpha smooth muscle actin
A disintegrin-like and metalloproteinase domain with thrombospondin type 1 motifs-like
Human adult cardiac fibroblast
Human foetal cardiac fibroblast
Hypertrophic obstructive cardiomyopathy
Large latent complex
Latent TGFβ binding protein
Small latent complex
Transforming growth factor beta
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We are grateful to the animal facility staff for excellent technical assistance.
This work was supported by the Research Council of Norway, Anders Jahre’s Fund for the Promotion of Science; the South-Eastern Regional Health Authority; the Kristian Gerhard Jebsen Foundation; and the Olav Raagholt and Gerd Meidel Raagholt`s Fund for Science, Norway to [I.G.L]; and the Allen Distinguished Investigator Program, through support made by The Paul G. Allen Frontiers Group and the American Heart Association to [S.S.A].
The authors declare no competing interests.
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Rypdal, K.B., Erusappan, P.M., Melleby, A.O. et al. The extracellular matrix glycoprotein ADAMTSL2 is increased in heart failure and inhibits TGFβ signalling in cardiac fibroblasts. Sci Rep 11, 19757 (2021). https://doi.org/10.1038/s41598-021-99032-2