Lung Research, Institute of Science and Technology in Medicine, University Hospital of North Staffordshire/Keele University, Stoke on Trent ST4 7NQ, Staffordshire, United Kingdom
Submitted 18 December 2003 ; accepted in final form 6 August 2004
![]() |
ABSTRACT |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
idiopathic pulmonary fibrosis; fibroblasts; statins; small GTPase
Statins are widely used as antilipidemic agents due to their efficacy in lowering low-density lipoprotein; they also have excellent tolerability and safety (23). The statins are known to interfere with the rate-limiting step of cholesterol biosynthesis; hence, they are first-line therapies for treatment and/or prevention of hypercholesterolemia. However, statins also appear to have a myriad of other cellular effects, including immunomodulation (6) and anti-inflammatory actions (20), which occur independently of their cholesterol-lowering abilities.
The statins abrogate the cholesterol synthesis pathway by inhibiting the enzyme 3-hydroxy-3-methylglutaryl coenzyme A (HMG CoA) reductase. However, the cholesterol pathway is also involved in small guanosine triphosphatase (GTPase) signaling. The isoprenoids farnesylpyrophosphate (FPP) and geranylgeranylpyrophosphate (GGPP), intermediates of the cholesterol synthesis pathway, are important lipid attachments for the posttranslational modification of proteins (32). Indeed, the small GTPases of the Rho and Ras family require posttranslational modification to enable them to bind to the cell membrane and exert signaling activities (18). Thus disruption of GTPase signaling could partly explain the emerging modulatory actions of statins on immune effector cells.
Data are now emerging that could implicate HMG CoA reductase inhibitors, otherwise known as statins, as having potential beneficial effects in the pathogenesis of fibrosis (8). The antifibrotic actions may result from disruption of small GTPase signaling, arising from inhibition of isoprenylation. This is supported by the observation that the small GTPases of the Rho family are important for basal as well as induced ccn2 (CTGF) expression in human renal mesangial cells (12). Indeed, HMG CoA reductase inhibitors were shown to interfere with the isoprenylation and subsequent activation of Rho proteins, resulting in modulation of CTGF expression, a downstream target of small GTPase activity. Consequently, we rationalize that such concepts could be applied to the overexpression of CTGF associated with IPF, although neither the in vitro nor in vivo use of statins in the lung has been documented to date.
In this present study, utilizing primary human normal and IPF-derived lung fibroblasts, we explore whether simvastatin can modulate CTGF gene and protein expression and, crucially, its induction by the profibrogenic mediator TGF-. Simvastatin is an inhibitor of the enzyme HMG CoA reductase, a key enzyme in the cholesterol synthesis pathway. As modulation of CTGF expression is thought to depend on the inhibition of the cholesterol synthesis pathway, specifically the signaling function of the small GTPases (16), we deliberately explore the role for the small GTPase Rho. Experimental culture models will incorporate transient transfection of a CTGF promoter reporter construct to establish the mechanisms used by simvastatin to exert its actions on the CTGF molecule. Accordingly, selective inhibitors (C3 exotoxin) and intermediates (GGPP and FPP) of the signaling pathways downstream of HMG CoA reductase, the enzyme known to be inhibited by simvastatin, will be utilized. Final confirmational experiments involve the transient transfection of dominant-negative and constitutively active RhoA constructs.
![]() |
METHODS |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
Experiments were carried out in normal human lung fibroblasts (IMR90, obtained from the American Type Culture Collection, Rockville, MD) and three separate human lung fibroblasts cell lines isolated from IPF patients [LL29 and LL97a from ATCC, Manassas, VA; and HIPF, a generous gift from R. J. McAnulty, University College London (UCL), London, UK]. IPF-derived cell lines in culture exhibit a more flattened dendritic morphology and enhanced expression of -smooth muscle actin (SMA) (3). Fibroblasts were cultured in Dulbecco's modified Eagle's medium (DMEM). Medium was supplemented with penicillin-streptomycin (100 U/ml; GIBCO-BRL, Paisley, UK) and L-glutamine (2 mM, GIBCO-BRL) with 10% fetal calf serum (FCS; Labtech, Sussex, UK). For experiments, medium was replaced with serum-free DMEM (SF-DMEM) for 48 h to induce quiescence before treatment. Human recombinant TGF-
1 (R&D Systems, Oxford, UK) was used at a dose of 5 ng/ml.
pLuc-CTGF Plasmid
pLuc-CTGF reporter vector (generous gift of Professor Eugene Chen, Morehouse School of Medicine, Atlanta, GA) encodes the CTGF promoter sequence, which is used to control the expression of the luciferase gene. With the CTGF gene sequence (GenBank accession no. AL354866), primers were designed to amplify the 2-kDa region relating to the CTGF promoter (bp 2,065 to +72) and were subsequently cloned into the luciferase reporter plasmid PGL3 (11) (Promega, Madison, WI).
Transient Transfections and CTGF Promoter Activity Assays
Transfections of human CTGF promoter-reporter constructs into human lung fibroblasts (HIPF) (at 90% confluence) were performed using the Transfast mammalian transfection system (Promega, Southampton, UK) following the manufacturer's recommendations. Cells were transfected with 0.75 µg of DNA per well (18-mm diameter) using a 1:1 ratio of DNA/Transfast reagent in serum-negative cultures. Confluent cells were incubated in the transfection mix containing the pLuc-CTGF plasmid for a 1 h; DMEM containing 10% FCS was added up to a volume of 1 ml, and cultures were left for 4 h. After this, the transfected cells were serum deprived for 48 h before treatment. After appropriate time points the cells were lysed, and luciferase activity was measured as chemiluminescence with a Berthold Lumat LB9501 luminometer (Berthold, Bad Wildbad, Germany) using the Steady Glo luciferase assay system (Promega). These data are presented as relative light units ± SE. Transfection efficiency was optimized and assessed using transfection of a plasmid construct containing green fluorescent protein (pEGFP-C1; Clontech, Palo Alto, CA). The cell density, DNA/Transfast ratio, and time course were optimized in repeated separate experiments; the optimized protocol was then used in subsequent transfection studies.
Dominant-Negative RhoA Transfections
Transfection of dominant-negative and constitutively active human RhoA (accession no. L25080) constructs into human lung fibroblasts (IPF-derived and IMR90 cells) were performed using the Transfast mammalian transfection system (Promega) as described above. RhoA G14V (a construct containing a mutation at G14V to render it constitutively active) and RhoA T19N (a construct containing a mutation at T19N, giving it a dominant-negative phenotype) constructs were utilized in a cDNA3.1+ vector and were obtained from the Guthrie Research Institute (www.cdna.org).
Treatment of Transfected HIPF Lung Fibroblasts
Simvastatin (Merck Sharp and Dohme, Hertfordshire, UK) was dissolved and filter sterilized before use (21). Quiescent, transfected HIPF lung fibroblasts were incubated for 16 h with simvastatin in SF-DMEM at a range of concentrations of 0.110 µM. After simvastatin preconditioning, cells were stimulated with TGF-1 (5 ng/ml) for 1 h. GGPP and FPP (Sigma Aldrich, Dorset, UK) were used at a concentration of 10 µM. Transfected cells were incubated for 16 h with these intermediates with and without the presence of simvastatin before 5 ng/ml TGF-
treatment for 1 h. Clostridium botulinum C3 exotoxin (Upstate Biotechnologies, Lake Placid, NY) was used at concentrations ranging from 0.5 to 5 µg/ml. Transfected cells were incubated with C3 exotoxin for 16 h before TGF-
(5 ng/ml) stimulation for 1 h. The concentration of TGF-
used in our experiments was determined from ongoing studies within the laboratories, in which 5 ng/ml were found to show significant induction of CTGF.
CTGF Gene Detection by Competitive RT-PCR
Quiescent, near-confluent IMR90 and HIPF lung fibroblasts were treated for up to 24 h with 5 ng/ml TGF-1 (R&D Systems). mRNA abundance was quantified by an established competitive RT-PCR procedure (5), using the primers shown in Table 1. The primers for the target genes were designed with computer assistance using Primer 3 (Whitehead Institute for Biomedical Research, Cambridge, MA). Primers were amplified within the coding region of the gene and spanned introns from the genomic template.
|
CTGF Gene Detection by Quantitative Real-Time RT-PCR
cDNA samples isolated from normal and IPF-derived lung fibroblasts transfected with the T19N and G14V RhoA constructs were used to assess CTGF gene expression. Two microliters of undiluted cDNA were used per reaction; a standard curve for CTGF and -actin was generated from serial dilutions of positively expressing cDNA. The probe and primer sets were "predesigned assay on demand" probes (Applied Biosystems, Foster City, CA); these predesigned primers are tested and standardized for reproducible expression analysis. Primer and cDNA were added to Taqman universal master mix (Applied Biosystems, Foster City, CA) containing all the reagents for PCR. Absolute quantification of the PCR products was carried out using the ABI prism 7000 (Applied Biosystems, Foster City, CA).
CTGF Protein Detection by Western Blotting
Total cell proteins were extracted in lysis buffer comprising 1% (vol/vol) Triton X-100, 20 mM Tris·HCl (pH 8.0), 10% (vol/vol) glycerol, 1 mM sodium orthanadate, 2 mM EDTA, 1 mM phenylmethylsulfonyl fluoride (PMSF), 20 µM leupeptin, and 0.15 U/ml aprotinin. Briefly, cells recovered by trypsinization were lysed in 30 µl of buffer and placed on ice for 20 min. The lysates were then centrifuged at 10 000 g for 15 min at 4°C to pellet cell debris. Supernatant containing the protein was recovered and assayed for total protein using a commercial microplate assay (Bio-Rad, Hemel Hempstead, UK). We combined 25 µg of total protein with sample buffer and boiled it for 5 min before gel loading. Proteins were resolved on a 12.5% polyacrylamide gel by electrophoresis at 120 V for 90 min in reducing buffer, and transfer was carried out at 100 V for 4 h. Membranes were blocked with 5% (wt/vol) BSA in Tris-buffered saline-Tween 20 (TBS-T) buffer overnight at 4°C. For detection of the CTGF protein a rabbit monoclonal anti-CTGF antibody (provided by FibroGen) was used at 2 µg/ml in TBS-T and 1% BSA for 1 h with gentle agitation. Secondary detection was carried out with a peroxidase-conjugated goat anti-rabbit IgG antibody (Jackson Immunoresearch, Philadelphia, PA) at a dilution of 1:25 000 in TBS-T and 1% (wt/vol) BSA for 1 h. The CTGF protein band was visualized by enhanced chemiluminescence (ECL; Amersham Pharmacia Biotech, Buckinghamshire, UK) according to the manufacturer's recommendations. Ponceau S staining of blots after transfer revealed equivalent loading of total protein; additionally, the membranes were reprobed for vinculin using antivinculin Ab-1 (clone VLN01, Labvision).
CTGF Protein Detection by Immunofluorescence
Treated lung fibroblasts were washed and fixed in situ in ice-cold methanol for 5 min. A primary rabbit monoclonal anti-human CTGF antibody (Fibrogen) was used (at 2 ng/ml in PBS, 30-min incubation at room temperature) to detect CTGF protein in fixed lung fibroblasts. After being washed thoroughly with PBS, a secondary antibody, anti-rabbit-FITC-conjugated IgG raised in sheep (Sigma Aldrich, Dorset, UK), was used at 1:1,000 dilution in PBS for 30 min at room temperature. Samples were mounted with Vectashield mounting media containing 4',6'-diamidino-2-phenylindole (DAPI; Vector Laboratories, Peterborough, UK). Slides were viewed under epifluorescence with a filter set at 450490 nm for FITC and 340380 nm for DAPI. Images were obtained using a Leica DC200 digital camera and software (Leica Microsystems, Heerbrugg, Switzerland). Camera exposure setting remained constant throughout the experiment; for each treatment, the total number of cells positive for CTGF expression was counted according to the published procedure (33). Five separate random fields of view were selected and imaged for each treatment, allowing the mean number of positively stained cells per field of view ± SE to be calculated.
Cell Viability
Cell viability was determined by Trypan blue (Sigma Aldrich, Dorset, UK) exclusion and accumulation of lactate dehydrogenase (LDH). LDH (a stable cytosolic enzyme that is released upon cell damage) was measured using a sensitive cytotoxicity detection kit (Roche, East Sussex, UK) following the manufacturer's recommendations.
Statistical Analysis
Data are shown as means ± SE. An unpaired Student's t-test was employed for comparing two groups of data. Multiple comparisons were made using analysis of variance, followed by Tukey's pair-wise comparison. All P values < 0.05 were considered significant.
![]() |
RESULTS |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
The expression of the CTGF gene was quantified in IMR90 and HIPF lung fibroblasts by competitive RT-PCR in response to treatment with simvastatin (0.1, 1, and 10 µM) (Fig. 1). Under exponential growth there is a 33.3% increase in basal CTGF expression in HIPF cells compared with IMR90. As expected, these levels of expression decrease following serum deprivation for 48 h; during this time the cells become quiescent. Serum-deprived cells were exposed to simvastatin; in both cell lines the drug induced further substantial decreases in CTGF gene expression at all concentrations. These results show that simvastatin can significantly downregulate (P < 0.05) CTGF gene expression even under basal conditions. Although the results shown are those from HIPF fibroblast cultures, the same pattern of simvastatin downregulation was also seen in the other two IPF-derived (LL29 and LL97a) fibroblast lines.
|
CTGF gene expression.
The effect of cell preincubation with varying concentrations of simvastatin (0.1, 1, 5, and 10 µM) on TGF- (5 ng/ml) induction of CTGF expression was evaluated in IMR90 and HIPF lung fibroblasts by competitive RT-PCR (Fig. 2). Compared with the untreated controls, TGF-
induced abundant upregulation in CTGF gene expression in both cell lines, more so in the HIPF (P < 0.05). However, fibroblast preconditioning with simvastatin for 16 h, before the TGF-
stimulation, was shown to override this TGF induction and downregulate CTGF gene expression in a concentration-dependent manner to subbasal levels. This inhibition of CTGF was significant in both fibroblast lines compared with equivalent cells treated with TGF-
alone at 1, 5, and 10 µM simvastatin (P < 0.05). Indeed levels of CTGF expression at the higher drug concentrations were decreased to below those exhibited in untreated resting cells. These observations suggest that simvastatin can maintain its downregulation of the CTGF molecule and abolish the potent stimulatory capacity of TGF-
in lung fibroblasts. Comparable results were also observed in the additional IPF-derived lung fibroblast lines (LL29 and LL97a).
|
|
The viability of lung fibroblasts following treatment remained uncompromised by simvastatin treatment as determined by trypan blue exclusion, with 89% of cells remaining viable even at the highest simvastatin concentration. In addition, measurement of the stable cytoplasmic enzyme LDH that is released rapidly into the supernatant upon cellular damage revealed that cytotoxicity remained <16% throughout our experiments (data not shown).
Effect of Simvastatin on CTGF Promoter Activity
To examine the mechanisms driving the actions of simvastatin on the CTGF molecule, cells from both IPF-derived and normal lung fibroblast lines were transfected with the pLuc-CTGF reporter construct. We performed all transfections using an in-house optimized procedure. The effects of varying concentrations of simvastatin on CTGF induction alone and in the presence of TGF- (5 ng/ml) were analyzed.
We observed that transfection of the pLuc-CTGF plasmid itself enhances the activity of the CTGF promoter by 80.7 and 90.2% in IMR90 and HIPF, respectively; these levels thus represented basal CTGF expression in the lung fibroblasts. Fibroblast preconditioning with simvastatin (0.110 µM) reduced the activity of the CTGF promoter. This was most pronounced at a drug dose of 10 µM, where a 36.8 and 34.9% reduction in luciferase release was observed in IMR90 and HIPF, respectively, compared with equivalent transfected, untreated cells; these changes are not significant (P < 0.08, Fig. 4A).
|
Effect of GGPP on CTGF Promoter Activity
GGPP is an intermediate of the cholesterol synthesis pathway and is involved in the postmodification of the small GTPase Rho. GGPP was employed to elucidate whether the cholesterol pathway was involved in simvastatin-induced responses of the CTGF gene. A significant increase (P < 0.05) in luciferase release from cells transfected and exposed to 5 ng/ml TGF- compared with transfected, untreated cells is observed (Fig. 5). However, as previously shown, pretreatment of cells with 10 µM simvastatin decreases luciferase release (P < 0.05); consequently, CTGF promoter activity is inhibited in the presence of simvastatin. GGPP alone was able to significantly elevate luciferase output from transfected cells compared with those preconditioned with simvastatin (10 µM) in all fibroblast cell lines used. GGPP was able to restore CTGF promoter activity in simvastatin-treated cells at all simvastatin concentrations used (0.1 and 1 µM simvastatin, data not shown). In those cultures preconditioned with 10 µM simvastatin, GGPP (10 µM) is able to restore CTGF promoter activity, increasing luciferase release by 44.6 and 68.9% over GGPP-negative equivalent cultures in IMR90 and HIPF, respectively. GGPP significantly increases the luciferase output from cells, with luciferase readings comparable to those observed from transfected, TGF-
-stimulated cells. These data implicate the cholesterol synthesis pathway and highlight in particular the crucial role of the intermediate GGPP in CTGF signaling.
|
|
In the above experiments, GGPP was able to effectively reverse the inhibitory effects induced by simvastatin on the CTGF gene. We concluded that geranylation of the small GTPase Rho is implicated in the signaling of CTGF. However, we also reasoned that the observed restoration of CTGF activity may not be specific to geranylation of Rho and could represent a generic action associated with the small GTPase family. To determine this, FPP (an intermediate involved in the farnesylation of the small GTPase Ras) was analyzed for its ability to restore CTGF promoter activity following simvastatin cell preconditioning. The addition of FPP was not able to produce significant induction of the CTGF promoter in all fibroblast lines used, suggesting that FPP, as well as the farnesylation with which it is involved, is not a critical activity in CTGF induction (data not shown). These findings confirmed that geranylation and therefore Rho signaling are essential to CTGF activity, whereas farnesylation and the associated signaling of Ras are not.
Use of C3 Exotoxin to Confirm the Role of Rho Signaling Pathway in CTGF Modulation
Clostridium botulinum C3 exotoxin (Upstate Biotechnologies) is an enzyme that specifically ADP ribosylates and inactivates Rho. The data presented previously revealed that geranylation of Rho and not farnesylation of Ras is important in induction of the CTGF promoter and therefore CTGF activity. The selective Rho inhibitor C3 exotoxin was employed to elucidate whether inhibition of Rho is able to influence CTGF promoter activity, modulating CTGF/TGF- interaction.
All tested concentrations (0.55 µg/ml) of C3 exotoxin significantly suppressed the luciferase release from TGF- in transfected cells (P < 0.05, Fig. 7A). At 5 µg/ml C3 exotoxin treatment, luciferase levels return to basal levels as seen in transfected, untreated cells. The results suggest that this selective inhibitor of Rho isoforms A, B, and C is able to inhibit the CTGF promoter activity, a response that is TGF-
independent. Importantly, C3 exotoxin itself does not show any significant alteration in the luciferase release compared with the control untransfected cells; therefore, treatment with this toxin does not alter the plasmid activity. In addition, levels of CTGF protein expression following C3 exotoxin treatment are also reduced (as shown by immunofluorescent cytology, Fig. 7B). Compared with samples treated to 5 ng/ml of TGF-
alone, there is a 24.9 and 14.8% reduction in the percentage number of IMR90 and HIPF cells expressing the CTGF protein, respectively, when they are treated with 5 µg of C3 exotoxin before TGF-
stimulation. Similar data were obtained in additional IPF-derived cell lines (LL29 and LL97a). Representative images of lung fibroblasts treated with C3 exotoxin are shown in Fig. 7C; the fluorescent intensity is greatly reduced following C3 exotoxin treatment, an observation most pronounced at 5 µg/ml. Interestingly, the viability of fibroblasts used in these experiments was not compromised by the addition of C3 exotoxin, with cytotoxicity determined by LDH release remaining <12% (data not shown).
|
Transient transfection of dominant-negative RhoA (RhoA T19N) and constitutively active RhoA (RhoA G14V) constructs was utilized to confirm the regulatory role of Rho in CTGF induction (Fig. 8). These data reveal that there is no significant difference between untransfected cells stimulated with TGF- alone compared with those transfected with the constitutively active RhoA construct. When constitutively active RhoA cultures are conditioned with TGF-
, there is a small but insignificant rise in CTGF gene expression. These data support a role for RhoA in CTGF induction; this is further confirmed by the use of a dominant-negative RhoA construct. Transfection of the RhoA T19N construct induces significant reduction (P < 0.05) in CTGF gene expression, producing a 63.0 and 38.6% reduction in IMR90 and IPF-derived lung fibroblasts, respectively, compared with cells stimulated with TGF-
alone; comparable levels are observed with cells transfected with RhoA G14V. There is, however, a slight but insignificant downregulation of CTGF gene expression in RhoA T19N ± TGF-
-treated cells (40.1 and 2.5% reduction in IMR90 and IPF-derived lung fibroblasts, respectively, compared with TGF-
treatment alone). We believe that this is a result of the transient transfection method; TGF-
is a known potent inducer of CTGF; in fact, we show that TGF-
alone is able to induce CTGF gene expression by 83.9% in HIPF lung fibroblasts. The transfection efficiency usually ranges from 35 to 40%, and thus even if Rho signaling is successful, the majority of the fibroblasts are still responsive to TGF-
. These data therefore reveal that by preventing functional RhoA expression, CTGF induction is reduced, supporting the concept of RhoA signaling in this process. Data shown for the HIPF fibroblast cultures also reflect the same pattern of findings as in the other two IPF-derived lung fibroblasts lines studied (LL29 and LL97a).
|
![]() |
DISCUSSION |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
Simvastatin is a member of the statin group, which are widely used in clinical practice because of their efficacy in the prevention of cardiovascular events (28), resulting in improved lipid profiles. However, it is increasingly recognized that statins have pleiotropic effects beyond that of cholesterol lowering. Recent reports have described the potential use of simvastatin in blocking CTGF action (12) and its antifibrotic potential (8) in renal disease. Hitherto such actions and associated underlying mechanisms of simvastatin on lung-derived fibroblasts have not been explored.
In this paper, we report that simvastatin can significantly inhibit CTGF gene expression in primary human lung fibroblasts; this was observed to occur parallel to a reduction in CTGF protein levels. Interestingly, the finding that basal CTGF expression in fibroblasts can be inhibited suggests that simvastatin can exert inhibitory effects on CTGF gene transcription.
TGF-, a recognized potent inducer of CTGF, produced a 73.1% induction of the CTGF gene in IMR90 normal lung fibroblasts and an 83.9% induction in HIPF lung fibroblasts. However, preconditioning of the same cells with simvastatin dose dependently inhibited TGF-
stimulatory effects, thereby lowering CTGF gene expression to below basal levels at 5- and 10-µM simvastatin concentrations. The data demonstrate the ability of simvastatin to modulate the TGF-
/CTGF interaction and specifically to override the potent induction of CTGF by TGF-
. In further support we have demonstrated that by using transient transfections of a plasmid construct containing the CTGF promoter sequence, simvastatin (0.110 µM) reduced the activity of the promoter irrespective of the presence of TGF-
in both normal and IPF-derived lung fibroblasts.
The cholesterol synthesis pathway is known to be inhibited by simvastatin. However, this pathway also possesses important signaling properties involving the small GTPases, which include the Ras, Rho, and Rac family. The small GTPase Rho has been implicated in normal wound healing (15); in addition, it has been suggested that guanine nucleotide-binding regulatory proteins (G proteins) are a novel signaling pathway able to induce CTGF in rat mesangial cells (16). Further elucidation of this pathway suggests that HMG CoA reductase inhibitors (statins) can inhibit the expression of the profibrotic mediator CTGF by interfering with the isoprenylation of small GTPases, specifically the isoprenylation of Rho (8). We incorporated intermediates of the cholesterol synthesis pathway in our series of experiments to establish the role of the small GTPases in the simvastatin-induced responses of the CTGF gene. The ability of GGPP to reverse the simvastatin-induced inhibition of the CTGF promoter activity, whilst FPP was unable to do so, suggests that the effects were not generic to the GTPases family and implicates a specific, crucial role for Rho. This was further substantiated by the use of C3 exotoxin (a specific inhibitor of Rho). The use of this reagent significantly inhibited CTGF promoter activity, irrespective of TGF- action; in addition C3 exotoxin was able to lower protein expression, thereby suggesting that Rho is essential for TGF-
-induced elevation of CTGF. To further clarify this link, dominant-negative and overexpression technology was utilized. Transient transfection of dominant-negative RhoA construct T19N resulted in a significant decrease in CTGF gene expression, whereas overexpression of RhoA using the G14V construct increased CTGF gene expression to levels comparable to those seen with TGF-
alone. We conclude that the modulatory effects of simvastatin on CTGF/TGF-
interactions (including its ability to inhibit CTGF expression) depend upon blocking Rho prenylation and its subsequent signaling.
Dysregulation of CTGF expression may be a key factor in influencing disease progression in IPF and consequently causing severe, irreversible lung parenchymal remodeling associated with fibrogenesis. It is possible that such events could be averted by the use of simvastatin. Indeed, utilizing a specifically designed in vitro cell model, we have carried out separate preliminary studies that have explored functional effects of simvastatin on -SMA gene and protein expression and collagen gel contraction. We have observed that simvastatin modulation of the CTGF molecule is associated with inhibitory changes in
-SMA expression and decrease in collagen gel contraction (K. L. Watts, unpublished observations).
-SMA and contractile properties are known to be associated with the myofibroblasts phenotype, a key element in fibrogenesis (19). From the current study data, we conclude that these antifibrotic effects of simvastatin arise from inhibition of Rho signaling and that Rho-like GTPases play a critical role in activation of TGF-
and its downstream pathways (30), including CTGF induction in fibrogenesis. If our preliminary functional data can be further elucidated, then the key question to be addressed in future would be whether simvastatin can have a pivotal role in averting crucial events leading to fibrosis development in vivo.
![]() |
GRANTS |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|
![]() |
ACKNOWLEDGMENTS |
---|
![]() |
FOOTNOTES |
---|
The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
![]() |
REFERENCES |
---|
![]() ![]() ![]() ![]() ![]() ![]() ![]() |
---|