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Tropomyosin 2.1 collaborates with fibronectin to promote TGF-β1-induced contraction of human lung fibroblasts

Respiratory Research volume 22, Article number: 129 (2021) Cite this article

Abstract

Many lung diseases are characterized by fibrosis, leading to impaired tissue patency and reduced lung function. Development of fibrotic tissue depends on two-way interaction between the cells and the extra-cellular matrix (ECM). Concentration-dependent increased stiffening of the ECM is sensed by the cells, which in turn increases intracellular contraction and pulling on the matrix causing matrix reorganization and further stiffening. It is generally accepted that the inflammatory cytokine growth factor β1 (TGF-β1) is a major driver of lung fibrosis through the stimulation of ECM production. However, TGF-β1 also regulates the expression of members of the tropomyosin (Tm) family of actin associating proteins that mediate ECM reorganization through intracellular-generated forces. Thus, TGF-β1 may mediate the bi-directional signaling between cells and the ECM that promotes tissue fibrosis. Using combinations of cytokine stimulation, mRNA, protein profiling and cellular contractility assays with human lung fibroblasts, we show that concomitant induction of key Tm isoforms and ECM by TGF-β1, significantly accelerates fibrotic phenotypes. Knocking down Tpm2.1 reduces fibroblast-mediated collagen gel contraction. Collectively, the data suggest combined ECM secretion and actin cytoskeleton contractility primes the tissue for enhanced fibrosis. Our study suggests that Tms are at the nexus of inflammation and tissue stiffening. Small molecules targeting specific Tm isoforms have recently been designed; thus targeting Tpm2.1 may represent a novel therapeutic target in lung fibrosis.

Introduction

In the western world, fibrosis is a major etiological factor in an estimated 45% of deaths [1] and interstitial lung diseases typified by fibrosis, including idiopathic pulmonary fibrosis (IPF), are significant contributors to global disease burden [2]. Increased extracellular matrix (ECM) secretion and deposition by tissue-resident fibroblasts (and other cells) increases tissue stiffness that characterizes fibrosis in IPF [3]. Moreover, fibroblasts pull on the ECM via forces exerted through the cellular actin cytoskeleton and this too can lead to increased tissue stiffening [4]. In previous studies, the inflammatory mediator TGF-β1 has been shown to induce ECM deposition [5, 6]. In separate studies, TGF-β1 has been shown to increase expression of the actin-associating tropomyosin (Tms) that are required for cells to exert force on the external environment [7]. We sought to determine whether TGF-β1 induces concomitant ECM deposition and Tms in human lung fibroblasts, thereby generating a feed-back loop that promotes tissue fibrosis.

Tissue desmoplasia (growth of fibrous or connective tissue) is initiated through large-scale ECM structural deregulation causing increased ligand density, fibril attachment and crosslinking, sustained by unregulated production of growth factors, cytokines and secretion of atypical matrix components. Damaged epithelial, endothelial and smooth muscle cells (and other structural cells) release cascades of inflammatory mediators. These mediators promote increased platelet formation, vasodilation, the stimulation of collagen-secreting fibroblasts and the secretion of matrix-metalloproteinases that degrade and reorganize the ECM. Cells sense the external tissue mechanical features by exerting intracellular-derived forces on the matrix generated by myosin-motor mediated contraction of bundles F-actin (stress fibres) [8]. The stress fibers are coupled via adaptor proteins to the cytoplasmic tail of ECM-bound integrins and ‘pull’ on ECM fibers on the external cell surface through the integrins [9]. The magnitude of the force required to deform the ECM by the cell is therefore related to the ECM stiffness and, in this manner, cells probe and respond to the mechanical forces in local tissue. A key aspect of the fibrotic circuit is the ability of the cells to sense forces in the external environment and to then contribute to the stiffening of the external tissue by relaying corresponding force onto the ECM [4]. Tms decorate the actin filaments and the specific isoform regulates the contractile function of the associated actin filament [10]. The Tm isoform Tpm2.1 is an example of a Tm that stabilizes actin stress fibres and thereby increases the contractile force derived through the stress fibres and exerted onto the surrounding tissue. Previous studies have shown that TGF-β1 induces Tpm2.1 [11], but this has not previously been reported in human lung fibroblasts. In this study, we focus on Tpm2.1 (an isoform coded from the TM1 gene) along with other key Tm isoforms associated with actin stabilization coded from the TM1 (Tpm1.6, Tpm1.7) and TM3 (Tpm3.1) gene.

IPF is characterized by excessive ECM deposition causing the lung parenchyma to stiffen, resulting in the progressive loss of lung function. While anti-fibrotic therapeutics, such as nintedanib and pirfenidone, have shown promise [12], a greater understanding of the underlying molecular mechanisms that underpin fibrotic progression may yield novel therapeutic targets. Despite a recognition that fibroblasts play a key role in pathogenesis and tissue dysfunction in pulmonary fibrosis, most studies to date have focused on the molecules and pathways that regulate ECM production, and in particular those induced by the pro-fibrotic inflammatory mediator, transforming growth factor β1 (TGF-β1). TGF-β1 is clearly a therapeutic target in IPF and other fibrotic conditions. However, treatment approaches targeting TGF-β1 signaling has proved challenging due to its integral role in health. These obstacles may prove to be overcome by innovative dosing regimens or other interventions [13].

Notably, a recent study revealed that in response to TGF-β1, lung fibroblasts showed greater cytoskeletal reorganization and importantly lung fibroblasts from IPF patients were stiffer when compared to control [14], suggesting that increased cellular stiffness may contribute to IPF pathology. Similar studies by Sarna et al. demonstrated change in stiffness of cells derived from people with asthma [15], underscoring the importance of fibrosis in respiratory diseases more broadly. Thus, in this study we test whether, in addition to its well-established ability to induce expression of the ECM fibronectin [5, 6], TGF-β1, also increases tropomyosin expression in human lung fibroblasts. We profile tropomyosin isoform and ECM production following TGF-β1 treatment and measure the functional outcomes by collagen gel contraction.

Materials and methods

Cell culture

Human lung fibroblasts were isolated from the parenchyma of lungs obtained from patients undergoing lung transplantation or surgical resection for thoracic malignancies, in accordance with procedures approved by the Sydney South West Area Health Service. Tables 1 and 2 show patient characteristics. Human lung fibroblasts were dissected and purified as previously described [16, 17]. Primary human fibroblasts were cultured in Dulbecco’s Modified Eagles Medium (DMEM) supplemented with 5% heat-inactivated fetal bovine serum, 0.5 mM L-glutamine, 20 mM HEPES and 1000 units/mL of penicillin, 1000 µg/mL of streptomycin, and 2.5 µg/mL of amphotericin B. All cells were seeded at 1.3 × 104 cells/cm2, cultured for 48 h and underwent quiescence (DMEM supplemented with 0.1% bovine serum albumin, 0.5 mM L-glutamine, 20 mM HEPES and 1,000 units/mL of penicillin, 1,000 µg/mL of streptomycin, and 2.5 µg/mL of amphotericin B) for 24 h prior to experimentation. All cell cultures tested negative for mycoplasma prior to experimentation and only cell cultures at less than 6 passages were used.

Table 1 Summary of patient demographics (for Fig. 5)
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Table 2 Summary of patient demographics (Fig. 8)
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Chemicals and reagents

Human recombinant TGF-β1 was from BioLegend (San Diego, CA). Type I collagen (rat tail) was from ThermoFisher Scientific (Waltham, MA). Custom-designed siRNA against Tpm2.1 siRNAs were purchased from Qiagen (Germantown, MD), comprising sequences targeting human Tpm2.1 (5′-AAGCACATCGCTGAGGATTCA-3′). Scrambled control sequences for knockdown experiments were Qiagen Allstar Non-targeting Control siRNA (Qiagen). Knockdown was achieved through siRNA transfection with Lipofectamine 2000 (Life Technologies, Carlsbad, CA). Unless otherwise specified, all chemicals used in this study were purchased from Sigma Aldrich (St. Louis, MO).

Real-time RT-PCR

Total RNA was extracted using the RNeasy Mini Kit (Qiagen) and reverse transcription performed by using the RevertAid First strand cDNA Synthesis kit (Fermentas Life Sciences, Hanover, MD) according to the manufacturer’s protocol. Real-time RT-PCR was performed on an ABI Prism 7500 with fibronectin 1 (Hs01549976_m1) TaqMan gene expression assays and GAPDH (Hs02786624_g1) as the endogenous control probe (Applied Biosystems, Foster City, CA) subjected to the following cycle parameters: 50 °C for 2 min, 1 cycle; 95 °C for 10 min, 1 cycle; 95 °C for 15 s, 60 °C for 1 min, 40 cycles and mRNA expression quantified by delta delta Ct calculations.

Protein extraction, SDS-PAGE and Western blotting

Adherent cells were lysed in 0.1% sodium dodecyl sulphate-RIPA buffer (containing protease inhibitors), sheared through a 26G syringe and needle, before centrifuging the lysate to remove the pellet. Protein concentration was measured by BCA assay and equal concentrations of protein added to the SDS-PAGE gels (fibronectin (6% gels)—10 µg protein applied; Tm isoforms (6% gels)—5 µg protein applied). Western blotting for fibronectin was performed with mouse monoclonal antibodies (clone IST-4: Sigma-Aldrich), compared to HSP-70 as the loading control (clone BRM-22: Sigma-Aldrich). Tm isoforms were detected with mouse monoclonal antibodies (generously provided by Peter Gunning, University of New South Wales) against Tpm1.6, Tpm1.7 and Tpm2.1 (α/9d) and Tpm3.1 (γ/9d) antibodies [7], compared to α-tubulin as the loading control (clone DM 1A, Santa Cruz Biotechnology). The choice of loading control (i.e. HSP-70 (~ 70 kDa) for fibronectin (~ 200 kDa) and α-tubulin (~ 55 kDa) for TM isoforms (~ 30 kDa)) was dictated by the molecular weight of the protein of interest and the relative mobility in either 6% or 12% SDS-PAGE, respectively, as the Western blots were reprobed for loading controls. Primary antibodies were detected with goat anti-mouse horseradish peroxidase–conjugated secondary antibodies (Cell Signaling Technology, Danvers, MA) and visualized by enhanced chemiluminescence (PerkinElmer, Wellesley, MA). Densitometry was performed with ImageJ [18].

Collagen gel contraction assay

Collagen gel contraction assays were performed by adapting previous publications [19, 20]. Briefly, 1 × 105 human lung fibroblasts in media (as above) were seeded within 1.3 mg/mL collagen (rat tail Type I) gels. Cells were incubated for 48 h at 37 °C. The cells then underwent quiescence for 24 h at 37 °C and the gels released from the wells by running a sterile yellow tip around the side of the well. Gels were left untreated (control) or stimulated with TGF-β1 (2 ng/mL) and images taken at 0, 24, 48, 72 and 96 h using a Kodak Imager. Triplicate technical replicates were performed and collagen gel area at each time point measured by ImageJ [18].

Tpm2.1 siRNA

Human lung fibroblasts were plated for 24 h before transfection (using Lipofectamine 2000) with siRNA against Tpm2.1 or scrambled control (Non-targeting Control siRNA) (both at a final concentration of 50 nM) for 24 h, as per previous publication [21]. Cells then underwent collagen gel contraction assay (as above) to determine the impact of knocking down Tpm2.1 on contraction at 0, 24, 48, 72 and 96 h. Knockdown was confirmed by Tpm2.1 Western blot (compared to HSP-70 as a loading control) and densitometry performed independently for all experiments.

Statistical analysis

Statistical analysis was performed with GraphPad Prism 8 using Student's unpaired t test and two-way ANOVA then Bonferroni’s multiple comparison test or multiple linear regression (least squares). P values < 0.05 were sufficient to reject the null hypothesis for all analyses. A 3D scatter plot was generated in R.

Results

TGF-β1 increases fibronectin mRNA expression and protein expression

While it is well established that the cytokine TGF-β1 increases fibronectin expression in human lung fibroblasts [5, 6], our first aim was to determine the temporal kinetics of TGF-β1-induced fibronectin mRNA expression in human lung fibroblasts. These are important foundational experiments to establish the conditions for further exploration. Cells were either untreated (vehicle control) or stimulated with TGF-β1 (2 ng/mL) for 0, 1, 4, 8, 24, and 48 h and fibronectin mRNA expression was quantified by real-time RT-PCR. No significant increase in fibronectin mRNA was detected within the first 8 h of TGF-β1 stimulation (Fig. 1). However, following TGF-β1 stimulation for 24 h a significant increase in fibronectin mRNA expression was observed (3.8 ± 0.8-fold) and sustained at 48 h (5.1 ± 1.6-fold) (P < 0.05) (Fig. 1). To determine if TGF-β1 also induced fibronectin protein expression, Western blot analysis was conducted following 24 and 48 h of TGF-β1 stimulation. Untreated cells show a small, but not significant, increase in fibronectin protein over time in untreated cells (Fig. 2). In comparison, TGF-β1 induced an increase in fibronectin protein at both 24 and 48 h post-stimulation (Fig. 2a) and densitometric analysis confirmed that TGF-β1 significantly increased fibronectin protein upregulation at 48 h (4.3 ± 1.1-fold) (P < 0.05) (Fig. 2b).

Fig. 1
figure 1

TGF-β1 increases fibronectin mRNA expression. Human lung fibroblasts were untreated (control) or stimulated with TGF-β1 (2 ng/mL) for 0, 1, 4, 8, 24 and 48 h. Fibronectin mRNA expression was quantified by real-time RT-PCR (results expressed as fold increase compared to control at 0 h). Statistical analysis was performed using two-way ANOVA then Bonferroni's multiple comparisons test (where * denotes a significant effect of TGF-β1 on fibronectin mRNA expression (P < 0.05)). Data are mean ± SEM values from n = 4–11 human lung fibroblast primary cell cultures

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Fig. 2
figure 2

TGF-β1 increases fibronectin protein upregulation. Human lung fibroblasts were left untreated (control) or stimulated with TGF-β1 (2 ng/mL) for 0, 24 and 48 h. Fibronectin protein upregulation was detected by Western blotting (compared to HSP-70 as a loading control). Results are shown as: a a representative Western blot; b densitometric analysis of fibronectin protein upregulation (normalised with HSP-70 and expressed as fold increase compared to control at 0 h). Statistical analysis was performed using two-way ANOVA then Bonferroni's multiple comparisons test (where * denotes a significant effect of TGF-β1 on fibronectin protein upregulation (P < 0.05)). Data are mean ± SEM values from n = 7 human lung fibroblast primary cell cultures

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TGF-β1 induces Tpm1.6/1.7 and Tpm2.1 protein expression

The impact of TGF-β1 on the multi-gene family of tropomyosins in this cell type was unknown. We address this herein, by performing Western blotting with two monoclonal antibodies: α/9d and γ/9d that detect specific isoforms coded by the TM1 (Tpm1.6, Tpm1.7 and Tpm2.1) and TM3 (Tpm3.1) genes, respectively. Human lung fibroblasts were treated with TGF-β1 or vehicle (control) for 24 and 48 h. Control primary fibroblasts showed no change in Tpm2.1 expression, and also showed no Tpm1.6 or Tpm1.7 expression over the time course (Fig. 3a). Conversely, TGF-β1-stimulated fibroblasts showed increased expression of Tpm2.1, Tpm1.6 and Tpm1.7 at both 24 and 48 h (Fig. 3a). Densitometric analysis revealed that stimulation with TGF-β1 for 48 h induced a significant 2.5-fold increase in Tpm2.1 (Fig. 3b) and 9.2-fold increase in Tpm1.6/1.7 isoforms (Fig. 3c; Tpm1.6 and Tpm1.7 isoforms were too close to analyze separately by densitometry and have therefore been grouped together and referred to as Tpm1.6/1.7) (P < 0.05). In contrast, Western blotting with γ/9d showed that TGF-β1 did not induce upregulation of Tpm3.1 (Fig. 4). Taken together, we show for the first time in human lung fibroblasts that TGF-β1 induces the protein expression of both fibronectin and those Tm isoforms encoded by the TM1 gene.

Fig. 3
figure 3

TGF-β1-induces protein upregulation of Tpm1.6/1.7 and Tpm2.1, but not Tpm3.1. Human lung fibroblasts were left untreated (control) or stimulated with TGF-β1 (2 ng/mL) for 0, 24 and 48 h. Tpm1.6/1.7 and Tpm2.1 protein upregulation was detected by Western blotting with the α/9d antibody, while Tpm3.1 was detected with the γ/9d antibody (compared to α-tubulin as a loading control). Results are shown as: a a representative Western blot; densitometric analysis of (b) Tpm2.1 and (c) Tpm1.6/1.7 protein upregulation (normalised with α-tubulin and expressed as fold increase compared to control at 0 h). Statistical analysis was performed using two-way ANOVA then Bonferroni's multiple comparisons test (where * denotes a significant effect of TGF-β1 on tropomyosin isoform upregulation (P < 0.05)). Data are mean ± SEM values from n = 7 human lung fibroblast primary cell cultures

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Fig. 4
figure 4

TGF-β1 does not induce upregulation of Tpm3.1 protein. Human lung fibroblasts were left untreated (control) or stimulated with TGF-β1 (2 ng/mL) for 0, 24 and 48 h. Tpm3.1 protein upregulation was detected by Western blotting with the γ/9d antibody (compared to α-tubulin as a loading control). Results are shown as: a a representative Western blot; b densitometric analysis of Tpm3.1 protein upregulation (normalised with α-tubulin and expressed as fold increase compared to control at 0 h). Data are mean ± SEM values from n = 10 human lung fibroblast primary cell cultures

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TGF-β1 induces human lung fibroblast-mediated collagen gel contraction

The ability of human lung fibroblasts to contract three-dimensional collagen gels is an in vitro model of ECM remodelling, a functional characteristic of lung fibrosis in vivo [22, 23]. To investigate the effects of TGF-β1 on human lung fibroblast-mediated collagen gel contraction, primary fibroblasts from n = 9 donors with a range of diagnoses (see Table 1) were used. Over the 96 h time course, fibroblasts stimulated with TGF-β1 displayed significantly increased contraction of the collagen gels from 48 h when compared to the vehicle control (Fig. 5: P < 0.05).

Fig. 5
figure 5

TGF-β1 induces human lung fibroblast-mediated collagen gel contraction. Collagen gel contraction assays mediated by human lung fibroblasts were performed by stimulating collagen gels with TGF-β1 (2 ng/mL) for 0, 24, 48, 72 and 96 h, in comparison to untreated controls. Results are expressed as collagen gel size (percentage compared to 0 h). Statistical analysis was performed using two-way ANOVA then Bonferroni's multiple comparisons test (where * denotes a significant effect of TGF-β1 on human lung fibroblast-mediated collagen gel contraction (P < 0.05)). Data are mean ± SEM values from n = 9 human lung fibroblast primary cell cultures

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TGF-β1-induced upregulation of fibronectin, Tpm1.6/1.7 and Tpm2.1 protein: inter-donor variability

While TGF-β1-induced fibronectin is a known contributor to the fibrotic lung fibroblast phenotype [23], the role TGF-β1-induced Tm expression plays in regulating collagen gel contraction was next assessed. Thus, parallel Western blot experiments were conducted using the same primary human lung fibroblasts used for the collagen gel contraction assay (Fig. 5). Fibroblasts were either left untreated (vehicle control) or stimulated with TGF-β1 for 0, 24 and 48 h. Protein levels of fibronectin (Fig. 6a), Tpm2.1 (Fig. 6b), Tpm1.6/1.7 (Fig. 6c) were quantitated and analysed by densitometry. The results are expressed as protein fold change compared to control t = 0 and are expressed for each donor (as well as the mean for the n = 9 donors at each time point). Although there was a significant impact of TGF-β1 on resultant protein levels (P < 0.05), not surprisingly, there was inter-donor variability between the TGF-β1-induced responses with TGF-β1 stimulating the fibroblast production of both fibronectin and Tms to different extents (Fig. 6). The biological variability is unsurprising given the range of disease diagnoses in the group of cell donors (Table 1). It is also important to note that the goal of the study was not to link disease to the resultant responses (and the study is not powered to do so). Rather, our aim was to examine cooperation between Tms and fibronectin on contractility of human lung fibroblasts. Accordingly, we next examined the possibility that TGF-β1-induced collagen gel contraction may be greater if TGF-β1 stimulation upregulates protein production of both fibronectin and TM1 isoforms.

Fig. 6
figure 6

TGF-β1-induced upregulation of fibronectin, Tpm1.6/1.7 and Tpm2.1 protein: inter-donor variability. Human lung fibroblasts were left untreated (control) or stimulated with TGF-β1 (2 ng/mL) for 0, 24 and 48 h. Western blotting was utilized to quantitate protein levels of: a fibronectin (compared to HSP-70 as a loading control); b Tpm2.1 (compared to α-tubulin as a loading control); c Tpm1.6/1.7 (compared to α-tubulin as a loading control)). Results shown are densitometric analysis (normalised to loading controls and expressed as fold increase compared to control at 0 h). Data are protein levels detected in human lung fibroblasts from each of the nine donors with mean represented as black bars. Statistical analysis was performed using two-way ANOVA then Bonferroni's multiple comparisons test (where * denotes a significant effect of TGF-β1 (P < 0.05))

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Tpm2.1 collaborates with fibronectin to promote TGF-β1-induced contraction of human lung fibroblasts

To address the possibility that fibrosis severity may be linked to the donor’s fibroblast response to TGF-β1 stimulation, we performed multiple linear regression to test the hypothesis that fibronectin may collaborate with one or more TM1 isoforms to regulate TGF-β1-induced collagen gel contraction. To do this, we represented the collagen gel contraction (from Fig. 5) as TGF-β1-induced collagen gel contraction (fold change over control at same time point) and measured area under the curve (AUC). With TGF-β1-induced collagen gel contraction (AUC) as the dependent variable, we conducted multiple linear regression to examine whether there was a statistically significant relationship between the dependent variable (contraction) and the explanatory variables (i.e. fibronectin and Tm isoforms) induced by TGF-β1. The model is represented as: Y = β0 + β1*B + β2*C; where Y is TGF-β1-induced collagen gel contraction (AUC); β0 is the intercept (constant term); β1 is the coefficient relating to B—TGF-β1-induced fibronectin protein upregulation at 48 h; β2 is the coefficient relating to C—TGF-β1-induced Tpm1.6/1.7 or Tpm2.1 protein upregulation at 48 h). There was no significant relationship (P = 0.5578) between TGF-β1-induced fibronectin and Tpm1.6/1.7 upregulation and resulting contraction (Y = 32.52 + 2.26*B – 0.38*C). In contrast, the combination of fibronectin and Tpm2.1 significantly predicted the extent of TGF-β1-induced contraction (Y = 56.99 + 9.174*B – 27.02*C: P = 0.0221). Thus, fibronectin together with Tpm2.1, but not Tpm1.6/1.7, promotes TGF-β1-induced contraction of human lung fibroblasts. This cooperative relationship is represented graphically in a 3D scatter plot (Fig. 7).

Fig. 7
figure 7

Tpm2.1 collaborates with fibronectin to promote TGF-β1-induced contraction of human lung fibroblasts. The relationship is represented graphically in a 3D scatter plot with the z-axis—TGF-β1-induced collagen gel contraction (area under the curve: AUC); x-axis—TGF-β1-induced fibronectin protein upregulation at 48 h; y-axis—TGF-β1-induced Tpm2.1 protein upregulation at 48 h

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Knocking down Tpm2.1 reduces human lung fibroblast-mediated collagen gel contraction

To demonstrate the importance of Tpm2.1 in human lung fibroblast-mediated collagen gel contraction, primary fibroblasts from n = 6 donors with a range of diagnoses (see Table 2) were transfected with siRNA against Tpm2.1 or scrambled control for 24 h. Cells then underwent collagen gel contraction assay and gel size in cells transfected with scrambled control or siRNA against Tpm2.1 measured at 0, 24, 48, 72 and 96 h. Knockdown was confirmed by Western blotting and, as shown in Figs. 8a and b, siRNA against Tpm2.1 reduced Tpm2.1 protein by 74.7 ± 5.3%, compared to scrambled control. Over the 96 h time course, knocking down Tpm2.1 significantly reduced human lung fibroblast-mediated collagen gel contraction, when compared to the scrambled control (Fig. 8c: P < 0.05).

Fig. 8
figure 8

Knocking down Tpm2.1 reduces human lung fibroblast-mediated collagen gel contraction. Human lung fibroblasts were transfected with siRNA against Tpm2.1 or scrambled control and collagen gel contraction measured at 0, 24, 48, 72 and 96 h. Tpm2.1 knockdown at 96 h was confirmed by Western blotting (compared to HSP-70 as a loading control). Results are shown as: a a representative Western blot; b densitometric analysis of Tpm2.1 protein (normalised with HSP-70 and expressed as percentage of scrambled control); (c) collagen gel size (percentage compared to 0 h). Statistical analysis was performed using (b) Student's unpaired t test and (c) two-way ANOVA then Bonferroni's multiple comparisons test (where * denotes that significantly knocking down Tpm2.1 protein represses human lung fibroblast-mediated collagen gel contraction (P < 0.05)). Data are mean ± SEM values from n = 6 human lung fibroblast primary cell cultures

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Discussion

Fibrotic tissue remodeling has a significant impact on morbidity and mortality worldwide. Treatment options are limited, and the fundamental mechanisms of disease progression are poorly understood. Thus, there is an urgent need to investigate fibrosis at the cellular and molecular level. The expression pattern of tropomyosin isoforms is critical, as the pattern of tropomyosin isoform decoration of actin filaments is a key determinant of the dynamics of the associated actin filament. We have shown that TGF-β1 induces the expression of Tpm1.6/1.7 and 2.1 and that via concomitant induction of Tpm2.1 and fibronectin protein expression, TGF-β1 induces human lung fibroblast-mediated collagen gel contraction.

During the fibrotic process, the actin cytoskeletons of fibroblasts in the tissue play a twofold role. Firstly, inflammatory cytokines induce enlarged actin fibers and focal adhesions. Secondly, the cells sense the increasing rigidity of the ECM by exerting traction forces through their focal adhesions (mechanosensing) and then convert this rigidity signal into increased actin fiber formation through the activation of biochemical signaling pathway (mechanotransduction) [24]. Increased actin fiber formation enables the cells to exert greater forces through the focal adhesions, which contracts the ECM and thereby disrupts the tissue structure [25]. Collectively, these changes to the fibroblast cellular structure therefore underpin the development of fibrosis. This interface of inflammation and mechanobiology is a key determinant of cellular architecture and tissue functioning. Currently, we do not fully understand why cells tip over into aberrant actin filament and focal adhesion formation to create the stiff, immobile fibroblast cells that are characteristic of fibrotic tissue. Intriguingly, a recent study by Jaffar et al. [14] demonstrated greater cellular stiffness in fibroblasts from people with IPF and greater cytoskeletal reorganization in response to TGF-β1. We propose that tropomyosins are key to actin stabilisation that characterize fibroblasts in fibrotic tissue.

Tropomyosins are a multi-isoform family of proteins that assemble into polymers and lay in the major groove of polymerized actin filaments [10]. The association of the tropomyosin polymer with actin filaments in turn determines the association of molecules that control actin filament turnover [26,27,28]. Ultimately, the pattern of tropomyosin decoration of actin filaments defines the function of the associated filament [29, 30]. The tropomyosin isoforms we have examined in this study have been associated with actin stabilisation, a key characteristic of cellular stiffening that occurs in fibrosis. Tpm1.6 stabilises stress fibres [31] and Tpm1.6/1.7 was recently shown to be recruited to actin filaments to increase actomyosin contractility [32]. Notably, the actin stabilizing role of isoform Tpm2.1 (previously known as Tm1) has previously led some investigators to describe it as a pro-fibrotic response gene [33]. Tpm3.1 (previously known as Tm5NM1) has been shown to stimulate actin stress fibre formation due to actin stabilisation [26, 34] in the context of cancer cell migration. Tm isoforms can exert distinct effects that depend on the cell’s physical environment (such as ECM) and thus it is important to note that cell- and disease-type differences can exist.

Tropomyosins are key players in actin dynamics and despite the key role of the actin cytoskeleton influencing fibrosis, surprisingly few studies have investigated the role of the pro-fibrotic cytokines TGF-β1 on tropomyosin expression, and none in lung fibroblasts from human subjects. Most studies to date have focused on the role and regulation of tropomyosins in TGF-β1-induced epithelial-mesenchymal transition in transformed epithelial cell lines (such as A549 [35], NMuMG [33, 36]) or primary lens epithelium [37, 38]. Schevzov et al. have shown that expression of Tm isoforms in human and mouse lung fibroblasts [7] and we are the first to extend these studies in human lung fibroblasts to show the inflammatory cytokine TGF-β1 also induce Tpm1.6/1.7, Tpm2.1, but not Tpm3.1.

We examined the hypothesis that cooperation exists between tropomyosin isoforms upregulated by TGF-β1 and fibronectin on the resultant collagen gel contraction, a model of lung stiffening [23]. We observed variability in patient specific expression of fibronectin, Tpm1.6/1.7 and Tpm2.1 induced by TGF-β1 (at 48 h) from n = 9 donors. Interestingly, multiple linear regression demonstrated a statistically significant relationship between the extent of Tpm2.1 and fibronectin induced by TGF-β1 and resultant collagen gel contraction. This would align with the known function of Tpm2.1 to stabilise actin and promote fibrosis [33], in addition to known ability of TGF-β1 to synthesise and deposit fibronectin into surrounding remodelled environment. Taken together, our results link Tpm2.1 to lung fibroblast stiffening that characterises fibrosis in IPF. However, while Fig. 7 offers a correlation between fibronectin, Tpm2.1 and TGF-β1-induced contractility, correlation need not mean causation. We conducted further experimentation (Fig. 8) to show that knocking down Tpm2.1 reduces human lung fibroblast-mediated collagen gel contraction.

Conclusion

At the interface of inflammation and mechanobiology, we propose that tropomyosins may play a role in controlling fibrotic development. Excitingly, selective Tm inhibitors are now in development [7, 39, 40], but their successful use in lung fibrosis first requires an in depth understanding of the inflammation-mediated regulatory networks that control tropomyosin isoform expression in lung fibroblasts. As modulation of tropomyosin isoform expression represents a tuneable approach towards controlling actin dynamics and cytoskeletal reorganization, the new knowledge gained by our study is essential for developing anti-fibrotic pharmacotherapeutic strategies for interstitial lung diseases in the future. Given that knocking down Tpm2.1 reduces human lung fibroblast-mediated collagen gel contraction, our data support the assertion that tropomyosins are tuneable actin-binding proteins at the interface of inflammation and mechanobiology and suggest that targeting Tpm2.1 may represent a therapeutic target in lung fibrosis.

Availability of data and materials

Available upon request.

References

  1. Wynn TA. Fibrotic disease and the T(H)1/T(H)2 paradigm. Nat Rev Immunol. 2004;4:583–94.

    Article  CAS  Google Scholar 

  2. Lee AS, Mira-Avendano I, Ryu JH, Daniels CE. The burden of idiopathic pulmonary fibrosis: an unmet public health need. Respir Med. 2014;108:955–67.

    Article  Google Scholar 

  3. Upagupta C, Shimbori C, Alsilmi R, Kolb M. Matrix abnormalities in pulmonary fibrosis. Eur Resp Rev. 2018;27:180033.

    Article  Google Scholar 

  4. Schwartz MA. Integrins and extracellular matrix in mechanotransduction. Cold Spring Harb Perspect Biol. 2010;2:a005066–a005066.

    Article  CAS  Google Scholar 

  5. Ignotz RA, Endo T, Massague J. Regulation of fibronectin and type I collagen mRNA levels by transforming growth factor-beta. J Biol Chem. 1987;262:6443–6.

    Article  CAS  Google Scholar 

  6. Dean DC. Expression of the fibronectin gene. Am J Respir Cell Mol Biol. 1989;1:5–10.

    Article  CAS  Google Scholar 

  7. Schevzov G, Whittaker SP, Fath T, Lin JJ, Gunning PW. Tropomyosin isoforms and reagents. Bioarchitecture. 2011;1:135–64.

    Article  Google Scholar 

  8. Kechagia JZ, Ivaska J, Roca-Cusachs P. Integrins as biomechanical sensors of the microenvironment. Nat Rev Mol Cell Biol. 2019;20:457–73.

    Article  CAS  Google Scholar 

  9. Elosegui-Artola A, Trepat X, Roca-Cusachs P. Control of mechanotransduction by molecular clutch dynamics. Trends Cell Biol. 2018;28:356–67.

    Article  CAS  Google Scholar 

  10. Gunning P, O’Neill G, Hardeman E. Tropomyosin-based regulation of the actin cytoskeleton in time and space. Physiol Rev. 2008;88:1–35.

    Article  CAS  Google Scholar 

  11. Bakin AV, Safina A, Rinehart C, Daroqui C, Darbary H, Helfman DM. A critical role of tropomyosins in TGF-beta regulation of the actin cytoskeleton and cell motility in epithelial cells. Mol Biol Cell. 2004;15:4682–94.

    Article  CAS  Google Scholar 

  12. Somogyi V, Chaudhuri N, Torrisi SE, Kahn N, Müller V, Kreuter M. The therapy of idiopathic pulmonary fibrosis: what is next? Eur Resp Rev. 2019;28:190021.

    Article  Google Scholar 

  13. Akhurst RJ. Targeting TGF-β signaling for therapeutic gain. Cold Spring Harb Perspect Biol. 2017;9:a022301.

    Article  Google Scholar 

  14. Jaffar J, Yang SH, Kim SY, Kim HW, Faiz A, Chrzanowski W, Burgess JK. Greater cellular stiffness in fibroblasts from patients with idiopathic pulmonary fibrosis. Am J Physiol Lung Cell Mol Physiol. 2018;315:L59-l65.

    Article  CAS  Google Scholar 

  15. Sarna M, Wojcik KA, Hermanowicz P, Wnuk D, Burda K, Sanak M, Czyż J, Michalik M. Undifferentiated bronchial fibroblasts derived from asthmatic patients display higher elastic modulus than their non-asthmatic counterparts. PLoS ONE. 2015;10:e0116840.

    Article  Google Scholar 

  16. Krimmer DI, Burgess JK, Wooi TK, Black JL, Oliver BGG. Matrix proteins from smoke-exposed fibroblasts are pro-proliferative. Am J Respir Cell Mol Biol. 2012;46:34–9.

    Article  CAS  Google Scholar 

  17. Rutting S, Zakarya R, Bozier J, Xenaki D, Horvat JC, Wood LG, Hansbro PM, Oliver BG. Dietary fatty acids amplify inflammatory responses to infection through p38 MAPK signaling. Am J Respir Cell Mol Biol. 2019;60:554–68.

    Article  CAS  Google Scholar 

  18. Schneider CA, Rasband WS, Eliceiri KW. NIH Image to ImageJ: 25 years of image analysis. Nat Methods. 2012;9:671–5.

    Article  CAS  Google Scholar 

  19. Wozniak MA, Keely PJ. Use of three-dimensional collagen gels to study mechanotransduction in t47d breast epithelial cells. Biol Proced Online. 2005;7:144–61.

    Article  CAS  Google Scholar 

  20. Matsumoto H, Moir LM, Oliver BG, Burgess JK, Roth M, Black JL, McParland BE. Comparison of gel contraction mediated by airway smooth muscle cells from patients with and without asthma. Thorax. 2007;62:848–54.

    Article  Google Scholar 

  21. Mitchell CB, Black B, Sun F, Chrzanowski W, Cooper-White J, Maisonneuve B, Stringer B, Day B, Biro M, O’Neill GM. Tropomyosin Tpm 2.1 loss induces glioblastoma spreading in soft brain-like environments. J Neurooncol. 2019;141:303–13.

    Article  CAS  Google Scholar 

  22. Fang Q, Liu X, Abe S, Kobayashi T, Wang XQ, Kohyama T, Hashimoto M, Wyatt T, Rennard SI. Thrombin induces collagen gel contraction partially through PAR1 activation and PKC-∈. Eur Resp J. 2004;24:918–24.

    Article  CAS  Google Scholar 

  23. Jin J, Togo S, Kadoya K, Tulafu M, Namba Y, Iwai M, Watanabe J, Nagahama K, Okabe T, Hidayat M, et al. Pirfenidone attenuates lung fibrotic fibroblast responses to transforming growth factor-beta1. Respir Res. 2019;20:119.

    Article  Google Scholar 

  24. Jansen KA, Donato DM, Balcioglu HE, Schmidt T, Danen EH, Koenderink GH. A guide to mechanobiology: where biology and physics meet. Biochim Biophys Acta. 2015;1853:3043–52.

    Article  CAS  Google Scholar 

  25. Hinz B. Formation and function of the myofibroblast during tissue repair. J Invest Dermatol. 2007;127:526–37.

    Article  CAS  Google Scholar 

  26. Bryce NS, Schevzov G, Ferguson V, Percival JM, Lin JJC, Matsumura F, Bamburg JR, Jeffrey PL, Hardeman EC, Gunning P, Weinberger RP. Specification of actin filament function and molecular composition by tropomyosin isoforms. Mol Biol Cell. 2003;14:1002–16.

    Article  CAS  Google Scholar 

  27. Ishikawa R, Yamashiro S, Matsumura F. Differential modulation of actin-severing activity of gelsolin by multiple isoforms of cultured rat cell tropomyosin. Potentiation of protective ability of tropomyosins by 83-kDa nonmuscle caldesmon. J Biol Chem. 1989;264:7490–7.

    Article  CAS  Google Scholar 

  28. Blanchoin L, Pollard TD, Hitchcock-DeGregori SE. Inhibition of the Arp2/3 complex-nucleated actin polymerization and branch formation by tropomyosin. Curr Biol. 2001;11:1300–4.

    Article  CAS  Google Scholar 

  29. Lees JG, Bach CT, O’Neill GM. Interior decoration: tropomyosin in actin dynamics and cell migration. Cell Adh Migr. 2011;5:181–6.

    Article  Google Scholar 

  30. Gunning PW, Hardeman EC, Lappalainen P, Mulvihill DP. Tropomyosin – master regulator of actin filament function in the cytoskeleton. J Cell Sci. 2015;128:2965–74.

    Article  CAS  Google Scholar 

  31. Tojkander S, Gateva G, Schevzov G, Hotulainen P, Naumanen P, Martin C, Gunning Peter W, Lappalainen P. A molecular pathway for myosin II recruitment to stress fibers. Curr Biol. 2011;21:539–50.

    Article  CAS  Google Scholar 

  32. Sao K, Jones TM, Doyle AD, Maity D, Schevzov G, Chen Y, Gunning PW, Petrie RJ. Myosin II governs intracellular pressure and traction by distinct tropomyosin-dependent mechanisms. Mol Biol Cell. 2019;30:1170–81.

    Article  CAS  Google Scholar 

  33. Gervasi M, Bianchi-Smiraglia A, Cummings M, Zheng Q, Wang D, Liu S, Bakin AV. JunB contributes to Id2 repression and the epithelial–mesenchymal transition in response to transforming growth factor–β. J Cell Biol. 2012;196:589–603.

    Article  CAS  Google Scholar 

  34. O’Neill GM. Scared stiff: stabilizing the actin cytoskeleton to stop invading cancer cells in their tracks. BioArchitecture. 2011;1:29–31.

    Article  Google Scholar 

  35. Tada A, Kato H, Takenaga K, Hasegawa S. Transforming growth factor beta1 increases the expressions of high molecular weight tropomyosin isoforms and vinculin and suppresses the transformed phenotypes in human lung carcinoma cells. Cancer Lett. 1997;121:31–7.

    Article  CAS  Google Scholar 

  36. O’Connor JW, Gomez EW. Cell adhesion and shape regulate TGF-Beta1-induced epithelial-myofibroblast transition via MRTF-A signaling. PLoS ONE. 2013;8:e83188.

    Article  Google Scholar 

  37. Kubo E, Shibata T, Singh DP, Sasaki H. Roles of TGF beta and FGF signals in the lens: tropomyosin regulation for posterior capsule opacity. Int J Mol Sci. 2018;19:3093.

    Article  Google Scholar 

  38. Shu DY, Lovicu FJ. Enhanced EGF receptor-signaling potentiates TGFbeta-induced lens epithelial-mesenchymal transition. Exp Eye Res. 2019;185:107693.

    Article  CAS  Google Scholar 

  39. Currier MA, Stehn JR, Swain A, Chen D, Hook J, Eiffe E, Heaton A, Brown D, Nartker BA, Eaves DW, et al. Identification of cancer-targeted tropomyosin inhibitors and their synergy with microtubule drugs. Mol Cancer Ther. 2017;16:1555–65.

    Article  CAS  Google Scholar 

  40. Janco M, Rynkiewicz MJ, Li L, Hook J, Eiffe E, Ghosh A, Böcking T, Lehman WJ, Hardeman EC, Gunning PW. Molecular integration of the anti-tropomyosin compound ATM-3507 into the coiled coil overlap region of the cancer-associated Tpm31. Sci Rep. 2019;9:11262.

    Article  Google Scholar 

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Acknowledgements

The authors wish to thank: our colleagues at the Woolcock Institute of Medical Research (especially Dikaia Xenaki and Brian Oliver); Jeff Hook and Peter Gunning (University of New South Wales); Amy Sarker and Victoria Prior (Children's Cancer Research Unit, Kids Research Institute, Children's Hospital at Westmead) and the collaborative effort of the cardiopulmonary transplant team and the pathologists at St. Vincent’s Hospital (Sydney, Australia), and the thoracic physicians and pathologists at the Royal Prince Alfred Hospital (Sydney) and Strathfield Private Hospital (Sydney, Australia).

Funding

The authors wish to acknowledge the generous support of the Ernest Heine Family Foundation, and Mrs Janice Gibson and the late Mr Freddie Gibson in establishing the Woolcock Emphysema Centre. This research is supported by an Australian Government Research Training Program Scholarship to PH and MR.

Author information

Author notes

  1. Geraldine M. O’Neill and Alaina J. Ammit—joint senior authors

Authors and Affiliations

  1. Woolcock Emphysema Centre, Woolcock Institute of Medical Research, University of Sydney, Sydney, NSW, Australia

    Peta Bradbury, Cassandra P. Nader, Aylin Cidem, Patrick He, Maria C. Rezcallah & Alaina J. Ammit

  2. School of Life Sciences, Faculty of Science, University of Technology Sydney, Sydney, NSW, Australia

    Peta Bradbury, Patrick He, Maria C. Rezcallah & Alaina J. Ammit

  3. Respiratory Cellular and Molecular Biology, Woolcock Institute of Medical Research, University of Sydney, Sydney, NSW, Australia

    Sandra Rutting

  4. Priority Research Centre for Healthy Lungs, Hunter Medical Research Institute and University of Newcastle, Newcastle, Australia

    Sandra Rutting

  5. Children’s Cancer Research Unit, Kids Research Institute, Children’s Hospital at Westmead, Sydney, NSW, Australia

    Dianne Sylvester & Geraldine M. O’Neill

  6. Children’s Hospital at Westmead Clinical School, Sydney, Australia

    Dianne Sylvester & Geraldine M. O’Neill

  7. School of Medical Sciences, Faculty of Medicine and Health, University of Sydney, Sydney, NSW, Australia

    Geraldine M. O’Neill

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Contributions

Conceived, designed and performed the experiments: PB, CN, AC, SR, PH, MR, GO’N, AA; analysis and interpretation: PB, DS, GO’N, AA; Wrote the paper: GO’N, AA. All authors read and approved the final manuscript.

Corresponding author

Correspondence to Alaina J. Ammit.

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Human lung fibroblasts were isolated from the parenchyma of lungs obtained from patients undergoing lung transplantation or surgical resection for thoracic malignancies, in accordance with procedures approved by the Sydney South West Area Health Service.

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Bradbury, P., Nader, C.P., Cidem, A. et al. Tropomyosin 2.1 collaborates with fibronectin to promote TGF-β1-induced contraction of human lung fibroblasts. Respir Res 22, 129 (2021). https://doi.org/10.1186/s12931-021-01730-y

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Keywords

Respiratory Research

ISSN: 1465-993X

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