Molecular Vision 2020; 26:742-756
Received 28 April 2020 | Accepted 23 November 2020 | Published 25 November 2020
1Harry S. Truman Memorial Veterans’ Hospital, Columbia, MO; 2One-Health Vision Research Program, Department of Veterinary Medicine & Surgery and Biomedical Sciences, College of Veterinary Medicine, University of Missouri, Columbia, MO; 3Mason Eye Institute, School of Medicine, University of Missouri, Columbia, MO
Correspondence to: Rajiv R. Mohan, Professor of Ophthalmology and Molecular Medicine, University of Missouri, 1600 E. Rollins St, Columbia, MO 65211; Phone+1-573-884-1449; FAX: +1-573-884-4100; email: email@example.com
Purpose: Inhibitor of differentiation (Id) proteins are helix–loop–helix (HLH) transcriptional repressors that modulate a range of developmental and cellular processes, including cell differentiation and cell cycle mobilization. The inhibitor of differentiation 3 (Id3) gene, a member of the Id gene family, governs the expression and progression of transforming growth factor beta (TGFβ)-mediated cell differentiation. In the face of mechanical, chemical, or surgical corneal insults, corneal keratocytes differentiate into myofibroblasts for wound repair. Excessive development or persistence or both of myofibroblasts after wound repair results in corneal haze that compromises corneal clarity and visual function. The objective of this study was to investigate whether Id3 overexpression in human corneal stromal fibroblasts governs TGFβ-driven cellular differentiation and inhibits keratocyte to myofibroblast transformation.
Methods: Primary human corneal stromal fibroblast (h-CSF) cultures were generated from donor human corneas. Human corneal myofibroblasts (h-CMFs) were produced by growing h-CSF in the presence of TGFβ1 under serum-free conditions. The Id3 gene was cloned into a mammalian expression vector (pcDNA3 mCherry LIC cloning vector), and the nucleotide sequence of the vector constructs was confirmed with sequencing as well as through restriction enzyme analysis. The Id3 mammalian overexpression vector was introduced into h-CSFs using a lipofectamine transfection kit. The expression of Id3 in selected clones was characterized with quantitative real-time PCR (qRT–PCR), immunocytochemistry, and western blotting. Phase contrast microscopy and trypan blue exclusion assays were used to evaluate the effects of the transfer of the Id3gene on the hCSF phenotype and viability, respectively. To analyze the inhibitory effects of the Id3 gene transfer on TGFβ-induced formation of h-CMFs, expression of the mRNA and protein of the myofibroblast marker alpha smooth muscle actin (α-SMA) was examined with qRT–PCR, western blotting, and immunocytochemistry. Student t test, analysis of variance (ANOVA), and Bonferroni adjustment for repeated measures were used for statistical analysis.
Results: The results indicate that Id3 overexpression does not alter the cellular phenotype or viability of h-CSFs. Overexpression of the Id3 gene in h-CSF cells grown in the presence of TGFβ1 under serum-free conditions showed a statistically significant decrease (76.3±4.3%) in α-SMA expression (p<0.01) compared to the naked-vector transfected or non-transfected h-CSF cells. Id3-transfected, naked-vector transfected, and non-transfected h-CSF cells grown in the absence of TGFβ1 showed the expected low expression of α-SMA (0–5%). Furthermore, Id3 overexpression statistically significantly decreased TGFβ-induced mRNA levels of profibrogenic genes such as fibronectin, collagentype I, and collagen type IV (1.80±0.26-, 1.70±0.35- and 1.70±0.36-fold, respectively; p<0.05) that a play role in stromal matrix modulation and corneal wound healing. Results of the protein analysis with western blotting indicated that Id3 overexpression in h-CSF cells effectively slows TGFβ-driven differentiation and formation of h-CMFs. Results for subsequent overexpression studies showed that this process occurs through the regulation of E2A, a TATA box protein.
Conclusions: Id3 regulates TGFβ-driven differentiation of h-CSFs and formation of h-CMFs in vitro. Targeted Id3 gene delivery has potential to treat corneal fibrosis and reestablish corneal clarity in vivo.
The loss of corneal transparency and the development of scars (haze) after ocular insults are the leading cause of global blindness [1-3]. The molecular mechanisms and cell-signaling pathways that play a role in the initiation or progression of corneal haze, and approaches for preventing pathological wound repair and promoting scar-free repair have been extensively studied using various experimental models [2-8]. We, and others, have found that numerous growth factors and cytokines command origination of wound-repairing myofibroblasts and the development of haze during corneal wound healing [2-8]. Corneal stromal fibroblasts grown in the presence of transforming growth factor β (TGFβ) under serum-free conditions express significantly increased level of α-smooth muscle actin (α-SMA), a myofibroblast biomarker [3-7]. TGFβ is a multifunctional cytokine that regulates many cellular processes, including wound healing, angiogenesis, proliferation, differentiation, and apoptosis after traumatic insult by modulating different types of transcription factors, including the runt-related transcription factor 1 (RUNX1, Gene ID: 600349, OMIM 151385), basic helix–loop–helix (BHLHE41, Gene ID: 600386, OMIM 606200), forkhead transcription factor (FOXE1, Gene ID: 600277, OMIM 602617), specificity protein 1 (SP1, Gene ID: 600581, OMIM 189906), activator protein 1 (JUN, OMIM 165160), and inhibitor of differentiation genes [9-12]. Furthermore, TGFβ influences more than 200 bHLH family members from yeast to humans . The bHLH proteins play an essential role in directing cell fate by regulating the transcription of various genes [13-15]. A conserved bHLH domain, consisting of two amphipathic helixes that facilitate homo- or heterodimerization or both is a distinctive feature of this family . Our previous studies exposed the association of transcriptional activity of bHLH proteins in TGFβ-driven fibrotic signaling in the cornea .
Inhibitor of differentiation proteins are DNA-binding transcription factors and have been implicated in the regulation of cell proliferation, migration, differentiation, inflammation, angiogenesis, and fibrosis [16-18]. Four Id genes (Id1 to Id4) exist in mammals, and we previously characterized the existence and expression of all four Id genes in the cornea . Members of the Id gene family have similar amino acid sequences within their HLH domain . Researchers revealed that Id proteins act as transcriptional regulators in a dominant-negative manner by dimerizing with unique bHLH transcription factors . The DNA binding activity of Id genes works as a functional inhibitor of bHLH transcription factors and regulates cell cycle progression. bHLH transcription factors control tissue-specific gene expression and regulate the transcription of target genes containing E-boxes in their promoters . Id proteins show unique spatiotemporal arrangements during development and cell cycle progression, although evidence indicates biochemical redundancy in vitro . The molecular mechanisms controlling Id protein expression are complex. Studies conducted during the last decade indicate that the transcription machinery of the Id gene is sensitive to stimulation from the extracellular environment, including cytokines like TGFβ, Smads, and BMP7 [2,5,21-23].
The Id3 (OMIM 600277) gene was first reported in 1991 in mice (GenBank Accession # 3399) and located on chromosome 1. It consists of three coding exons and two introns . The Id3 protein (15 kDa) is a member of the Id family of class V HLH proteins, which are 119 amino acids long . Various in vivo studies on mice have shown that Id3 plays a role in embryonic development through interaction with Id1 and Id2 [26,27]. In adult rodents, Id3 is an early responsive gene with expression levels increasing in response to growth factor stimulation . The Id3 protein, as implied by its name, was initially thought to be an inhibitor of cell differentiation [28,29]. Researchers contend that the loss or gain of Id protein function can lead to cellular makeover [20,30,31]. Id3 has been shown to be involved in the differentiation of many cell types, including fibroblasts, preadipocytes, and myofibroblasts [26-29]. However, recently the role of Id3 as a global differentiation blocker has been questioned [31-33].
In the cornea, our research indicates that the association between TGFβ hyperactivity and Idgenes regulates the transcriptional machinery during corneal wound healing. This prompted us to postulate that the overexpression of the Id3 gene in corneal stromal fibroblasts impede excessive myofibroblast generation in stroma and subsequent haze formation in the cornea. In this study, we examined whether overexpression of the Id3 gene can control TGFβ1-mediated corneal fibroblast differentiation and investigated the underlying mechanism using an in vitro human corneal fibrosis model.
An Institutional Review Board approved the study and the study adhered to the tenets of the Declaration of Helsinki and the ARVO statement on use of human donor tissues. Primary human corneal stromal fibroblasts (h-CSFs) were generated from donor human corneas obtained from an eye bank (Saving Sight, Kansas City, MO) using methods described previously . Briefly, the epithelial and endothelial layers of the corneal tissues were removed with mild scraping with a scalpel blade, and residual corneal tissue was washed with Minimum Essential Medium (MEM; Gibco, Life Technology Corp., Grand Island, NY). The corneal tissue was divided into small pieces, placed in 100 × 20 mm cell culture dishes (Corning Inc., Corning, NY) with MEM supplemented with 10% fetal bovine serum (Thermo Fisher Scientific, Grand Island, NY), and incubated at 37 °C in 5% CO2 for 3–5 weeks to obtain h-CSFs. h-CSF cells with 70% confluence were then used for experiments from two to five passages. Human corneal myofibroblast (h-CMF) cultures were produced by culturing h-CSFs in the presence of TGFβ1 (5 ng/ml; PeproTech Inc., Rocky Hill, NJ) under serum-free conditions, and cultures were incubated at 37 °C in 5% CO2 for 72 h.
To generate a mammalian expression vector-construct expressing the Id3gene, PCR-amplified human Id3 gene (Accession number NM_002167) product (about 950 bp) was cloned in pcDNA3 mCherry LIC mammalian expression vector using standard molecular biologic techniques . Restriction mapping and DNA sequencing were used to confirm the nucleotide sequence of the pcDNA3 mCherry Id3 vector construct and was termed Id3-transfected or Id3-mCherry for the entire study. Lipofectamine 3000 (Invitrogen, Life Technology Corp.) was used to deliver the Id3-mCherry plasmid into the h-CSF culture following the manufacturer’s instructions. Briefly, 250 µl of DNA-lipid transfection solution was added dropwise to each well of the six-well plate by mixing equal volumes (125 µl) of Lipofectamine 3000 (7.5 µl) and plasmid DNA (5 µg DNA in 10 µl P3000) diluted with Opti-MEM and incubated for 15 min at room temperature. Cultures were then incubated at 37 °C in a humidified CO2 incubator for 8 h, washed with Opti-MEM, and incubated for 72 h in MEM supplemented with 10% serum. The stably transfected clones overexpressing the Id3 gene were identified by subjecting the transfected cultures to gentamicin (G418 sulfate; 250–400 µg/ml) selection (Thermo Fisher) following the standard molecular biologic protocol.
To monitor and record cellular morphology and the phenotypic progression at various time points for the cells, a Leica DMIL phase contrast microscope equipped with the Leica DFC290 imaging system (Leica Microsystems Inc., Buffalo Grove, IL) was used. Trypan blue exclusion dye and 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) assays using the CellTiter 96® Non-Radioactive Cell Proliferation Assay Kit (Thermo Fisher) were performed to determine the cellular viability, growth, and proliferation profile of the cells following published protocols . Concisely, cells were trypsinized, and suspended in 0.4% trypan blue solution at various time points. Dead cells appeared blue as the dye entered the interior of the cells because of a broken membrane; live cells remained white due to intact membranes. Cell counts were performed with Neubauer’s counting chamber (Thermo Fisher), and cellular viability was calculated and expressed in percentage of live cells in culture. Viability assays were performed to monitor the cellular growth profile of Id3-delivered and un-delivered cells.
The RNeasy kit (Qiagen Inc., Valencia, CA) was used to extract mRNA from harvested cells and was reverse transcribed into cDNA using a commercial kit (Promega, Madison, WI) following the manufacturer’s instructions. Quantitative real-time PCR (qRT–PCR) was performed using All-in-One qPCR mix (GeneCopoeia, Rockville, MD) in accordance with the manufacturer’s instructions. Briefly, each 20 µl reaction contained 10 µl 2X All-in-One qPCR mix, 2 µl cDNA (0.5 µg), 2 µl forward primer (0.2 µM), and 2 µl reverse primer (0.2 µM), and 4 µl RNase and DNase free water and ran at a universal cycle (95 °C for 3 min, 40 cycles of 95 °C for 30 s followed by 60 °C for 60 s) following the published protocol . The nucleotide sequences of the primers (forward and reverse) used for amplification in this study are provided in Table 1. Beta actin (β-actin) was used as a housekeeping gene to normalize the qRT–PCR data and verify the quality of the cDNA. The threshold cycle (Ct) was used to detect the increase in the signal associated with exponential growth of the PCR product during the log-linear phase. The relative mRNA expression was calculated using the following formula, 2ΔΔCt. The ΔCt validation showed similar amplification efficiency for all templates used (the difference between linear slopes for all templates was less than 0.1).
To extract proteins, the cells were washed with ice-cold PBS (1X; pH 7.4; 137 mM NaCl, 2.7 mM KCl, 11.9 mM Phosphates) and lysed with a radioimmunoprecipitation assay (RIPA) buffer (50 mM Tris-HCl, pH 7.5, 150 mM NaCl, 1% NP-40, 0.5% sodium deoxycholate) containing a protease inhibitor mixture (Roche Applied Sciences, Indianapolis, IN). Debris and other residue were removed with centrifugation at 14,000 ×g at 4 °C, and clear protein lysate was collected for protein estimation using the Bio-Rad assay (Bio-Rad Life Sciences, Hercules, CA) .
Western blotting was performed using a standardized protocol . Briefly, protein samples in Laemmli’s sample buffer containing β-mercaptoethanol at 70 °C for 10 min were denatured. Proteins were resolved on 4–10% sodium dodecyl sulfate–polyacrylamide gel electrophoresis (SDS–PAGE) and transferred onto a 0.45 µm pore size polyvinylidene difluoride (PVDF) membrane using the Xcell-II blot module (Thermo Fisher). The membrane was blocked with 3% bovine serum albumin (BSA; Santa Cruz Biotechnology Inc., Dallas, TX) in Tris-buffered saline containing 0.1% Tween-20 detergent (TBST) for 1 h and probed with primary antibodies and housekeeping antibodies (1:100 dilution) in TBST followed by secondary anti-mouse or -goat antibodies (1:20,000 dilution). National Institutes of Health (NIH; (Bethesda, MD) ImageJ 1.38X image analysis software was used for digital quantification of detected protein bands using densitometry analysis.
Immunocytochemistry and fluorescence microscopy were performed to characterize and quantify α-SMA, a myofibroblast marker, to determine the levels of myofibroblasts and fibrosis using a mouse monoclonal antibody for α-SMA (Dako, Agilent Technologies, Carpinteria, CA). The Id3-delivered, naked-vector delivered, and normal h-CSF cells were grown in the presence or absence of TGFβ1 (5 ng/ml) under serum-free conditions for 72 h, fixed with 4% freshly prepared paraformaldehyde. For immunostaining, fixed cells were washed twice with ice-cold PBS and blocked with 2% BSA (SC2323, Santa Cruz Biotechnology). Mouse monoclonal antibody for α-SMA was used at a 1:200 dilution in 1X PBS for 90 min followed by secondary antibody Alexa 488 or 594 goat anti-mouse IgG (Invitrogen, Molecular Probes, Life Technologies Corp., Eugene, OR) at a dilution of 1:500 for 1 h. Cells were mounted with Vectashield containing 4′,6-diamidino-2-phenylindole (DAPI; Vector Laboratories, Burlingame, CA) for visualization of the nuclei. Irrelevant isotype-matched primary antibody, secondary antibody alone, and tissue sections from naïve eyes were used as negative controls. Stained cells were visualized under a Leica fluorescence microscope (Leica, Wetzlar, Germany) and photographed with a digital camera (SpotCam RT KE, Diagnostic Instruments Inc., Sterling Heights, MI). The α-SMA-stained cells in ten randomly selected areas were counted per 200X and 400X magnification field.
Statistical analysis was performed using GraphPad Prism 6.07 software (GraphPad, La Jolla, CA). Statistical evaluation was executed using the Student t test and one-way ANOVA (ANOVA) followed by the Bonferroni multiple comparison test for post-hoc analysis in different cellular and molecular assays. The experiments were performed in triplicate (unless stated differently), and results of experiments are expressed with standard deviation (SD). Results of the experiment were considered statistically significant if the p value was less or equal to 0.05 from the total population.
The quality of the cDNA and successful delivery of the plasmid-expressing Id3 gene in h-CSFs were confirmed with PCR amplification using primer sequences specific to the β-actin gene and the Id3-mCherry gene-insert cloned in the expression vector, respectively. Figure 1 shows an amplification product at 617 bp and confirmation of the presence of Id3-mCherry DNA in Id3-transfected cells. As expected, no amplification products (617 bp) were detected in the normal and naked-vector transfected cells. A band detected at 350 bp indicates the presence of β-actin, as the positive control. No amplification bands were detected in negative controls that had Id3-mCherry forward and reverse primers without cDNA.
Cultures were subjected to immunocytochemistry to confirm the success of the gene transfer and expression of the Id3-mCherry gene inserted in the h-CSFs. Figure 2 shows representative images illustrating the expression of an mCherry fluorescent marker protein in h-CSF cells transfected with the Id3-mCherry plasmid (Figure 2H,I) and the absence of the fluorescent marker protein in normal (non-transfected) and naked-vector transfected cells (Figure 2A–F).
The cellular morphology of normal, naked-plasmid vector transfected, and Id3-mCherry transfected h-CSFs was examined under phase contrast microscopy. As evident from Figure 3, transfer of the Id3 gene did not alter the cellular morphology of the h-CSFs. Normal and transfected h-CSF cultures had spindle-shaped, flattened, and elongated morphology with contacts to neighboring cells, which is typical of corneal stromal fibroblasts when grown in MEM supplemented with 10% fetal bovine serum. The lack of differences in the cellular morphology between the Id3-mCherry-delivered cells (Figure 3C) and the normal (Figure 3A) or naked-vector delivered (Figure 3B) cells suggests that overexpression of Id3 is nontoxic to h-CSFs.
Next, we determined the effects of overexpression of Id3 on h-CSF growth, proliferation, and viability using commercial assays. Figure 4 shows growth and proliferation profiles (Figure 4A), and cellular viabilities (Figure 4B) of normal, naked-vector delivered, and Id3-delivered h-CSFs. Screened Id3-delivered and naked-vector delivered h-CSFs showed growth patterns (Figure 4A), and cellular viability (Figure 4B) similar to those of the non-transfected or normal h-CSFs. As evident from the MTT data presented in Figure 4A, a non-statistically significant difference (4–8%; p>0.05) in the growth rate was observed among non-transfected or normal, naked-vector delivered, and Id3-delivered h-CSFs up to five tested passages. Furthermore, 94–98% cells were found viable in three cell types in the trypan-blue assay and up to five tested passages as evident in Figure 4B.
To study the effect of the Id3 gene on TGFβ1-stimulated cell differentiation and myofibroblast generation, cultures were grown in the presence or absence of TGFβ1 (5 ng/ml) under serum-free conditions and analyzed for changes in cellular morphology and myofibroblast biomarker α-SMA protein levels. The phase contrast images in Figure 5 show the extent of cellular differentiation in normal non-transfected, naked-vector transfected, and Id3-transfected h-CSF cultures. As expected, TGFβ1 treatment in normal h-CSFs (Figure 5D) and naked-vector transfected h-CSFs (Figure 5E) induced transdifferentiation and produced phenotypic characteristics of the myofibroblasts. Conversely, Id3-overexpressing h-CSFs under similar conditions resisted cellular differentiation and maintained typical fibroblastic morphological characteristics (Figure 5F). None of these cells grown in the absence of TGFβ1 underwent cellular differentiation and acquired the myofibroblast phenotype (Figure 5A–C). This phenomenon was further verified with immunofluorescence using an antibody specific for the α-SMA protein.
Figure 6 shows the levels of the α-SMA protein in the Id3-transfected and normal non-transfected h-CSFs grown in the presence or absence of TGFβ1 under serum-free conditions. As evident from the panels, the Id3-transfected h-CSFs show statistically significantly decreased α-SMA immunostaining (Figure 6D) compared to the normal non-transfected h-CSFs grown in the presence of TGFβ1 (Figure 6C), but neither the Id3-transfected h-CSFs nor the normal non-transfected h-CSFs show any detectable α-SMA levels when grown in the absence of TGFβ1 (Figure 6A,B). This suggests that the Id3 gene negatively regulates cellular differentiation and myofibroblast production. The α-SMA protein levels of the naked-vector controls were found to be analogous in normal or non-transfected h-CSFs (data not shown). Figure 7 shows quantification of TGFβ1-induced h-CSF differentiation to myofibroblasts by the Id3 gene, which was statistically significant (76.3±4.30%; p<0.001).
The impact of the Id3 gene during fibrosis was analyzed by measuring the relative change in mRNA expression of profibrotic genes in cells induced by TGFβ1 that underwent cell differentiation and myofibroblast production. The Id3-transfected and normal non-transfected h-CSFs were grown in the presence or absence of TGFβ1 under serum-free media and mRNA levels of four fibrotic genes in the extracellular matrix (ECM) and were quantified with qRT–PCR. Figure 8 shows the relative change in the mRNA expression of the ECM genes, namely, α-SMA, fibronectin, and collagentypesI and IV. TGFβ1 stimulation caused statistically significant increases in the expression of profibrogenic genes α-SMA (5.50±0.53-fold; p<0.001), fibronectin (3.10±0.26-fold; p<0.01), collagen type I (2.70±0.35-fold; p<0.01), and collagen type IV (2.20±0.36-fold; p<0.01) in normal, non-transfected h-CSFs. Id3-delivered h-CSFs significantly defied the TGFβ1-driven differentiation process, including the production of ECM components and profibrotic genes. Id3-transfected h-CSFs showed a statistically significant decrease in the mRNA levels of α-SMA (3.20±0.19-fold; p<0.001), fibronectin (1.80±0.26-fold; p<0.01), collagen type I (1.70±0.35-fold; p<0.01), and collagen type IV (1.70±0.36-fold; p<0.01) compared to those of normal, non-transfected h-CSFs under similar culture conditions (Figure 8). The mRNA levels of these genes in naked-vector transfected h-CSFs were found to be analogous to those of normal non-transfected h-CSFs.
To characterize the molecular mechanism of the Id3 gene on the cellular differentiation event, we investigated the interactions of Id3 with the bHLH region of the E2A protein. Normal, non-transfected and Id3-transfected h-CSFs were grown in the presence or absence of TGFβ1, and the levels of the α-SMA and E2A proteins were quantified with western blotting. Figure 9 shows the results of western blotting and quantification of the Id3, α-SMA, and E2A proteins under normal and TGFβ1 influence. The increased α-SMA and Id3 protein levels with the associated decrease in the E2A protein level in the Id3-transfected h-CSFs compared to normal non-transfected h-CSFs grown under the influence of TGFβ1 (Figure 9A) suggest that negative regulation of cellular differentiation occurs via interactions of Id3 with the bHLH region of the E2A protein. This notion was further supported by the observation that no noticeable changes were detected in the α-SMA and E2A protein levels, when these h-CSFs were grown in the absence of TGFβ1. The densitometry analysis of the western blotting data showed the decrease in the α-SMA (51.4±2.10%; p<0.001) and E2A protein levels (46.1±3.40%; p<0.001) in the Id3-transfected h-CSFs was statistically significant compared to that of the normal non-transfected h-CSFs (Figure 9B).
The overexpression of Id3 attenuates TGFβ1/Smad-driven cell differentiation through a dominant negative effect by the DNA binding of the E-protein bHLH region. In the present study, we showed direct biochemical evidence of HLH proteins, Id3 and E2A with fibrosis marker α-SMA. We proposed the molecular mechanism that the formation of hetero-oligomeric complexes of Id3 with the E-protein of bHLH would modulate the differentiation cascade in h-CSFs (Figure 10).
TGFβ is a member of a superfamily of polypeptides that regulates cell cycle progression, differentiation, and chemotaxis of many different types of cells [2,5]. TGFβ also regulates a diverse set of essential cellular processes during the development of corneal fibrosis [3-7]. In response to corneal insults, endogenous epithelial-derived TGFβ drives populations of keratocytes to transdifferentiate into myofibroblasts, initiating the process of corneal wound healing. The developed myofibroblast cells undergo cellular matrix remodeling and result in ECM disorganization with abundant collagen type III and IV populations that contribute to loss of corneal transparency. Differentiation events include the production of ECM proteins, mediation of cell adhesion, and modulation of collagen fibrillogenesis governed through TGFβ/Smad signaling . Ultimately, this leads to the development of corneal fibrosis. The information garnered from this study shows that overexpression of the Id3 gene inhibits TGFβ-modulated expression of profibrogenic genes and formation of myofibroblasts in h-CSFs.
Although several imminent novel TGFβ-responsive genes encoding transcription factors have been identified, in this study, we focused on the Id family of transcription factors, specifically Id3. Initial investigations of Id proteins focused on their role in development [27,36], and subsequent studies exposed a role for Id proteins in influencing many essential cellular functions, including cell proliferation, differentiation, survival, and invasion, along with angiogenesis, senescence, apoptosis, and metastasis [16-22]. Within Id proteins, the basic region of the bHLH protein is not present, and therefore, it cannot bind to the DNA directly. Id proteins have a dominant-negative effect by binding DNA bHLH proteins that drive cell lineage, commitment, and differentiation [37,38]. We previously reported the expression and role of Id1 to Id4 in human and rabbit normal and fibrotic corneas .
One trigger of the corneal fibrosis cascade is induction of reactive oxygen species (ROS) . Current literature shows that Id3 regulates the differentiation phenomenon through induction of ROS in vascular epithelial cells due to redox-sensitive properties [19,38-40]. The results of the present study demonstrate that overexpression of the Id3 gene in h-CSFs attenuates the impact of profibrotic cytokines and modulates cellular differentiation, as well as wound healing cascades. These results are well supported by previous studies performed in myocytes that showed overexpression of Id proteins delayed the onset of differentiation . The present study also revealed the underlying mechanism that the HLH proteins, Id3, and E2A can form hetero-oligomeric complexes that modulate the differentiation cascade. These findings corroborate many literature reports that showed Id proteins have the ability to act as an inhibitor of myofibroblast formation by associating with bHLH class A and E proteins (E12, E47, E2–2, and HEB) [41-45]. Conversely, other non-ocular studies reported the induction of Id3 expression by TGFβ, and this information suggests a role for Id3 in regulating the transcriptional responses of fibroblasts [21,43]. In this study, the mRNA and protein results indicate that Id3 overexpression controls TGFβ-mediated profibrotic events. The noticeable reduction in the mRNA expression of collagensI and IV in Id3-overexpressing cells suggests that Id3 plays an important role in corneal matrix organization and TGFβ-induced differentiation. Results of this study reflect that Id3 suppresses myofibroblast differentiation by controlling the bHLH protein. These findings correspond with preadipocyte literature and validate that Id3 either interacts directly with the bHLH protein or prevents the interaction of E2A proteins . Ids heterodimerize through HLH motifs, which are highly conserved within this protein family. It is conceivable that all other isoforms of Ids interact with the same protein-binding site to regulate the differentiation process. Constitutive expression of Id3 also stops differentiation in adipose cells, but the effect of other Id proteins (Id1, Id2, and Id4) on differentiation has not been examined . The protein data suggest a mechanistic role for Id3 and E-box proteins in the corneal fibroblast differentiation process; however, the data did not categorically establish a cause-and-effect relationship between the Id3 and E-box proteins. Our ongoing in vitro and in vivo studies characterizing mechanistic and functional roles of Id3 and E-box proteins on cellular differentiation of corneal fibroblasts will address this limitation, and fill gaps in knowledge. Furthermore, they are expected to exhibit whether suppression of TGFβ/Smad signaling by bHLH proteins through overexpression of the Id3gene into corneal stroma can offer clinically valuable modality to treat corneal opacity and restore corneal transparency in vivo.
Gene therapy in the cornea is a promising therapy for the prevention and treatment of visual disability due to corneal scarring . Additionally, gene therapy to treat corneal scarring has been successfully demonstrated by delivering genes with an adenosine-associated viral or nanoparticle vector into rabbit and human keratocytes [7,8,25]. The potential of Id3gene therapy to inhibit TGFβ-driven fibrosis has been reported in many non-ocular tissues employing various in vivo and in vitro models [21,29,32,33,44]. Our ongoing in vivo rabbit studies focus on developing gene therapies that reduce corneal scar or haze through the use of gain-of-function of Id3 overexpression by ectopic overexpression into corneal stroma to modulate the TGFβ/Smad signaling pathways.
In summary, overexpression of the Id3 gene downregulated profibrotic gene expression and effectively prevented TGFβ-driven transformation of h-CSFs into h-CMFs through the interaction of Id3 with the basic region of the TATA box E-box protein. Based on these results, Id3 gene therapy warrants further investigation as a conceivable treatment for corneal fibrosis in vivo.
This work was primarily supported by the 1I01BX000357, Veteran’s Health Affairs Merit and Research Career Scientist grants (RRM), Washington DC, USA; and partially by the NIH/NEI 5R01EY017294; 5R01EY030774, and 1U01EY031650 grants (RRM) Bethesda, Maryland, USA, and the Ruth Kraeuchi Missouri Endowed Chair Ophthalmology Fund (RRM) University of Missouri, Columbia, Missouri, USA.