Molecular Vision 2012; 18:874-886
Received 30 June 2011 | Accepted 4 April 2012 | Published 7 April 2012
Jennifer L. Winkler, Mamdouh H. Kedees, Yelena Guz, Gladys Teitelman
State University of New York, Downstate Medical Center, Department of Cell Biology, Brooklyn, NY
Correspondence to: Gladys Teitelman, State University of New York, Downstate Medical Center, Department of Cell Biology, 450 Clarkson Avenue Box 5, Brooklyn, NY; Phone: (718) 270-2950; FAX: (718) 270-3732; email: firstname.lastname@example.org
Purpose: Connective tissue growth factor (CTGF) is a profibrotic factor that induces extracellular matrix (ECM) production and angiogenesis, two processes involved in diabetic retinopathy (DR). In this study, we examined whether insulin therapy or a CTGF-specific small interfering RNA (siRNA) administered to diabetic rats decreased the levels of CTGF and of selected putative downstream genes in the retina.
Methods: Rats with streptozotocin-induced diabetes were used. Animals received either no treatment for 12 weeks or were administered constant insulin therapy. MRNA and protein levels of CTGF and select ECM genes were determined using real-time PCR and western blotting of the retina. Localization of CTGF in the retina was visualized using immunohistochemistry. A group of diabetic rats received intravitreal injection of CTGF siRNA, and the retinas were examined three days later.
Results: CTGF mRNA and protein significantly increased in the retinas of diabetic rats. Immunohistochemistry indicated that retinal Müller cells of diabetic rats expressed CTGF. Hyperglycemia upregulated mRNA levels of fibronectin, laminin β1, collagen IVα3, and vascular endothelial growth factor (VEGF), and this increase was prevented by insulin therapy. Treatment of diabetic rats with CTGF siRNA decreased laminin β1, collagen IVα3 mRNA, and CTGF mRNA and protein but did not affect fibronectin or vascular endothelial growth factor mRNA levels.
Conclusions: These results indicate that CTGF and ECM genes can be regulated using insulin. Importantly, these results also suggest that CTGF regulates changes in ECM molecules in DR.
Diabetic retinopathy (DR) is the leading cause of visual impairment and blindness among adults of working age in the United States . DR can be divided into two stages. The first stage is non-proliferative DR, characterized by retinal edema, microaneurysms, venous bleeding, and soft exudates. The second stage, proliferative DR, is characterized by angiogenesis, retinal detachment, blindness, and an increased number of blood vessels with altered vascular permeability. DR occurs because of altered blood flow, pericyte loss, tissue hypoxia, and basement membrane thickening provoked by increased production of collagen IV, laminin, and fibronectin [2-4]. These changes were detected after 12 and 17 weeks following the appearance of diabetes, respectively [5,6]. In addition, there is also dysregulation of remodeling proteins such as matrix metalloproteinease-2, matrix metalloproteinease-9 (MMP-9), plasminogen activator inhibitor-1, tissue inhibitor of metalloproteinease-1, and other proteins [7-9].
Connective tissue growth factor (CTGF) is a profibrotic factor that induces extracellular matrix (ECM) production and angiogenesis , two processes involved in the development of DR. CTGF is one of the six members of the CCN family of proteins. The CCN acronym is derived from the names of the first three members of the family of proteins: Cyr61 (cysteine-rich protein 61), CTGF, and NOV1 (nephroblastoma overexpressed gene-1). The CCN family of proteins is involved in a wide range of functional pathways such as cell adhesion, cell survival, angiogenesis, tumorigenesis, and wound healing . CTGF is upregulated in human and rodent models of DR [12,13] and is induced by glucose [5,13] and advanced glycation end-products . In addition, CTGF is upregulated by vascular endothelial growth factor (VEGF) [14,15], which is increased in patients with diabetes and is a critical regulator of vascular permeability and angiogenesis .
The exact role of CTGF in the progression of DR has yet to be determined. Although CTGF knockout is embryonic lethal , CTGF heterozygote mice have a 50% decrease in CTGF levels in plasma and urine and show decreased retinal basal lamina thickening in diabetes . In addition, CTGF is responsible for the development of fibrosis, not angiogenesis, which results in scarring of the retina and blindness . Studies of the kidney strengthened the possibility that CTGF mediates the alterations of ECM during hyperglycemia .
In this study, we sought to determine the role of CTGF in non-proliferative DR. First, we tested whether the increase in CTGF levels with hyperglycemia could be attenuated through insulin therapy and whether this treatment affected the level of expression of key ECM molecules. Since glycemic levels fluctuate during insulin therapy, we also tested whether a specific inhibition of CTGF using siRNA affects the levels of selected ECM molecules that increase in the diabetic retina.
Male Sprague Dawley Rats (Charles River, Troy, NY), weighing approximately 200 g, received a single (IP) injection of 80 mg/kg streptozotocin (STZ; Sigma, St. Louis, MO) dissolved in 0.1 M citrate buffer (pH 4.5) . Control non-diabetic animals were injected with an equal volume of citrate buffer. Fasting blood glucose (FBG) levels were measured using a PrecisionXtra blood glucose monitor (Abbot, Alameda, CA). Animals with FBG greater than 350 mg/dl were considered diabetic. The first day of recorded hyperglycemia was considered day 1 of the experiment. Animals were euthanized with Euthasol (120 mg/kg; Vibrac Corp., Fort Worth, TX) and sacrificed after 8 and 12 weeks of hyperglycemia. Eyes were enucleated, and the retina dissected in nuclease free ice-cold PBS (137 mM sodium chloride, 2.7 mM potassium chloride, 8 mM sodium phosphate dibasic, 2 mM potassium phosphate monobasic, pH 7.4). The animal procedures were in accordance with the institutional Animal Care and Use Committee and with the standards established by the New York State Department of Health, the USA Public Health Service, the USA Department of Agriculture, and the Association for Assessment and Accreditation of Laboratory Animal Care.
Rat-2 fibroblasts (ATCC, Manassas, VA) were maintained in vitro as previously described . Briefly, cells were maintained in Dulbeco’s Modified Eagle Medium (DMEM, Sigma) supplemented with sodium bicarbonate (1.5 g/l; Invitrogen, Carlsbad, CA) and 10% fetal bovine serum (FBS, Invitrogen). Rat-2 cells were seeded at a density of 5.8×105 cells in a T-25 tissue culture flask (Falcon; BD, San Jose, CA) and allowed to adhere overnight. Transfection agent (siPORT-Amine; Ambion, Austin, TX) was diluted (1:40) in Opti-MEM (Invitrogen) and incubated at room temperature for 10 min. Three CTGF siRNAs (Ambion) were individually tested for their effect on CTGF mRNA and protein. Sequences for these siRNAs are shown in Table 1. Each siRNA (50 mM), diluted in 900 µl of Opti-MEM, was added to the transfection mix and incubated at room temperature for 10 min. The siRNA/transfection agent complexes were added to suspended cells (1.8×106), and the mixture was placed in a T-75 flask in medium containing 10% FBS. siRNA transfected cells were incubated at 37 °C with CO2 for 24 h. Then the cells were processed and treated with transforming growth factor (TGF)-β1 (R&D Systems, Minneapolis, MN) as previously described . In brief, cells were incubated with 0.5% FBS DMEM medium containing TGF-β1 (0.1 ng/ml) for 4 or 6 h before harvesting. After TGF-β1 treatment, cells were trypsinized with 0.25% trypsin-EDTA (Trypsin-EDTA; Invitrogen) and pelleted by centrifugation at 200 g for 5 min (International Equipment Company, Chattanooga, TN). Cell pellets were washed in RNase-free ice-cold PBS and centrifuged at 1,300× g (MTX-150; Tomy Tech, Menlo, CA) for 10 min at 4 °C and then used for total RNA isolation or protein extraction.
A subset of diabetic animals (FBG≥350 mg/dl) was implanted with subcutaneous insulin pellets (LinShin Canada Inc., Toronto, Canada) for 12 weeks, on the first day of hyperglycemia according to the company’s recommendations. FBG was measured 1 week after insulin pellet implantation (day 1 of the experiment for the group treated with insulin), and weekly thereafter. Animals with poor glycemic control received two additional insulin pellets.
After 12 weeks of hyperglycemia, a subset of rats received a single intravitreal injection of siRNA. Animals were anesthetized with vaporized isoflurane. Eyes were visualized with a dissecting microscope, and the sclera was pierced behind the ora serrata using a borosilicate glass capillary (World Precision Instruments, Sarasota, FL) that was heat pulled to obtain a thin diameter. siRNAs (Table 1) were modified for in vivo studies by Dharmacon (Lafayette, CO), using undisclosed techniques due to proprietary considerations. siRNA was diluted in sterilized, RNase/DNase-free, physiologic PBS for a final concentration of 2.5 µg/µl. siRNA was injected using a sterilized Nanofill syringe attached to a 33G beveled needle (World Precision Instruments) inserted in the opening produced by the capillary needle. One eye was injected with 3 µl (7.5 µg) of CTGF siRNA and the contralateral eye with scrambled siRNA (7.5 µg). Animals were sacrificed at 3 and 10 days post siRNA injection.
To track and visualize siRNA inside the layers of the retina, a Label IT siRNA Tracker Kit (Mirus, Madison, WI) was used to label the scrambled siRNA with Cy3. Briefly, about 10 mg of siRNA (Silencer® Negative Control #2 siRNA; Ambion) was incubated with 5 μl labeling buffer A (Mirus) and 10 μl labeling reagent (Mirus) at 37 °C for 1 h, unreacted Label IT siRNA Tracker Reagent was removed from the labeled siRNA with ethanol precipitation, and labeled siRNA was spun, washed with ethanol 70%, and resuspended in PBS. Purified, labeled siRNA was quantified with spectrophotometry. Five μg (in 2 μl PBS) of labeled siRNA was injected in one eye. The contralateral eye was injected with the same volume of unlabeled siRNA. Eyes were enucleated 3 days later, placed in mounting medium, snap frozen in liquid nitrogen, and cryosectioned, and cells were visualized by staining the nuclei with To-Pro Blue (Invitrogen).
Animals were euthanized, and the eyes were immersed in embedding matrix (ThermoFisher, Waltham, MA) and snap frozen in liquid nitrogen. Then 20 µm sections were obtained. The plane of section was parallel to the optic nerve. Cryosections were fixed in ice-cold acetone (10 min), and post-fixed in Zamboni’s fixative for 2 min. Slides were washed in 0.1 M PBS, and sequentially incubated in PBS containing 0.3% hydrogen peroxide for 20 min, in blocking buffer (PBS containing 3% horse serum and 0.01% saponin) for 30 min, and incubated with goat anti-human CTGF antibody (diluted 1:100 in 0.01 M PBS; R&D) at 4 °C overnight. The specificity of this antibody has been previously described [22-26]. The next day, slides were incubated for 1 h with Alexa Fluor 488 conjugated with antigoat immunoglobulin G (diluted 1:200 in 0.01 M PBS; Invitrogen), washed in PBS, fixed in 4% paraformaldehyde for 5 min, and incubated overnight with mouse anti-vimentin antibody (1:500 in 0.01 M PBS). The following day, slides were incubated for 1 h with Alexa-Fluor 594 (1:200 in 0.01 M PBS; Invitrogen) and coverslipped using Vectashield mounting medium (Vector, Burlingame, CA).
Confocal images were obtained using a Radiance 2000 confocal microscope (Bio-Rad, Hercules, CA) connected to a Zeiss Axioskop microscope (Carl Zeiss, Thornwood, NY). Images of 1240×1240 pixels were processed using Photoshop (Adobe, San Jose, CA). All images were captured using similar settings on the confocal microscope.
Total RNA was extracted using the RNAeasy Kit (Qiagen, Germantown, MD) as described in Winkler et al. . Briefly, concentration and purity of RNA were determined by spectrophotometry. RNA integrity was verified by electrophoresis in 1.2% denaturing formaldehyde gel (1.2 g agarose, 10 ml 10× FA gel buffer [200 mM 3-[N-morpholino] propanesulfonic acid; MOPS], 50 mM sodium acetate, 10 mM EDTA, pH 7.0) in 100 ml RNase-free water). RNA preparations were treated with recombinant DNase-1 (DNA-free kit; Ambion). One microgram of total RNA was transcribed using SuperScript III reverse transcriptase and oligo(dT)18 primer (Invitrogen). Real-time PCR was performed using RT2 SYBR Green Mix (SA Biosciences, Frederick, MD) and performed on a StepOnePlus cycler (Applied Biosystems, Carlsbad, CA). The cycling conditions were 95 °C for 10 min, 40 cycles at 95 °C for 15 s, and 60 °C for 1 min. mRNA levels were normalized to an appropriate housekeeping gene, TATA-binding protein (TBP)  or acidic ribosomal protein P0 (ARPP0) . Primer sequences for laminin β1, fibronectin 1, and collagen IVα3 were taken from a previous publication . Details of the primers are shown in Table 2. Data was analyzed using the 2-∆∆C(T) method . Each sample was run in triplicate, and each real-time PCR was repeated three times.
Retinas were homogenized for 5 min in ice-cold lysis buffer (50 mM Tris HCl, pH 7.4, 5 mM EDTA, and 0.02% sodium azide) containing a cocktail of protease inhibitors (Sigma). After homogenization, samples were centrifuged at 28,000× g for 10 min at 4 °C. Protein concentration in cleared lysates was measured using bicinchoninic acid colorimetric assay (BCA kit; Pierce, Rockford, IL). Samples were fractionated on a 15% Tris-HCl sodium dodecyl sulfate–PAGE (SDS–PAGE) Ready Gel (Bio-Rad) for CTGF and VEGF and a 5% Tris-HCl SDS–PAGE Ready Gel (Bio-Rad) for laminin; 30 µg of total protein was loaded into each lane. After electrophoresis, protein samples were electroblotted onto nitrocellulose membrane (Amersham, Pittsburgh, PA), washed in Tris-buffered saline, and incubated overnight at 4 °C with goat anti-CTGF antibody (1:1,000; Santa Cruz, Santa Cruz, CA). Membranes were incubated with horseradish peroxidase–conjugated Donkey anti-goat secondary antibody (1:10,000; Santa Cruz), and bands were visualized using SuperSignal West Pico chemiluminescent detection reagents (Thermo Scientific) and Hyblot-CL Autoradiography Film (Denville, Metuchen, NJ). Membranes were subsequently stripped with Restore Western Blot Stripping (Thermo Scientific), incubated with antibodies to VEGF (1:1,000; Santa Cruz) and to glyceraldehyde 3-phosphate dehydrogenase (GAPDH; 1:1,000; Santa Cruz) for loading control, and processed for immunodetection as described as above. GAPDH was chosen because changes in protein levels have been reported in vivo only after 12 months of hyperglycemia . Different membranes were incubated with anti-laminin sera, a pan-specific antibody that recognizes multiple laminin isoforms (1:1,000; Novus, Littleton, CO). For loading controls, membranes were stained with Ponceau S. Densitometric analysis of the luminescent signal was performed at non-saturating exposures. Bands were scanned with Epson Perfection 2400 and analyzed using Image J software (NIH, Bethesda, MD). Densitometry was performed using proteins that were run on the same gel.
All values are shown as mean±SD. For comparison between two groups, the unpaired Student t test (two tail) was used. p≤0.05 was considered significant.
To ascertain whether CTGF gene expression increased during hyperglycemia, the level of CTGF mRNA and protein in the retina of diabetic and non-diabetic control rats was compared. At 8 and 12 weeks of hyperglycemia, CTGF mRNA was sixfold (p<0.05) and sevenfold (p<0.001) higher than in controls, respectively (Figure 1A and Figure 2A). Similarly, CTGF protein increased 2.5 fold (p<0.05) at 8 weeks and 5.7 fold (p<0.05) at 12 weeks of hyperglycemia (Figure 1B,C and Figure 2B,C). These findings are in agreement with previous reports by others [5,12,13]. To ascertain the identity of the cells expressing CTGF, sections of retina were processed for simultaneous visualization of CTGF and vimentin, a marker of Müller cells . This analysis indicated that in the retina of diabetic rats, CTGF is expressed by vimentin-positive Müller cells (Figure 3).
In addition to an increase in CTGF, hyperglycemia affected the level of expression of VEGF and of possible downstream ECM genes in the retina. Comparison of the retina of 12-week diabetic and normoglycemic rats revealed a significant increase in fibronectin (threefold, p<0.001), laminin β1 (2.5 fold, p<0.05), collagen IVα3 (2.3 fold, p<0.05), and VEGF (twofold, p<0.001) mRNAs (Figure 2A). Protein levels of VEGF and laminin also increased significantly (2.1 fold and 5.2 fold, respectively [p<0.05]) in the retina after 12 weeks of hyperglycemia (Figure 2D,E). These results confirm previous observations obtained using a similar model [4,32].
To ascertain whether insulin therapy affects the level of expression of CTGF, VEGF, and possible downstream ECM molecules in the retina, a subset of rats with STZ-induced diabetes received insulin therapy at 7 days post-STZ for 12 weeks. Insulin therapy normalized blood glucose levels and reduced weight loss in diabetic rats (Table 3). The levels of CTGF, fibronectin, laminin β1, collagen IVα3, and VEGF mRNAs in the retinas of diabetic rats receiving insulin therapy were similar to that of controls (Figure 2A). Similarly, CTGF, VEGF, and laminin proteins were similar in insulin-treated STZ and non-diabetic control (Figure 2B-E). To confirm the effect of insulin on CTGF, the levels of CTGF in the retinas of the control, diabetic, and insulin-treated diabetic rats were compared with immunohistochemistry. The level of CTGF immunostaining was undetectable in control retinas (Figure 4A), increased in diabetic retinas (Figure 4B), and significantly reduced in the retinas of diabetic rats treated with insulin (Figure 4C). In addition, we confirmed previous reports indicating that insulin treatment normalized fibronectin levels in the retinas of diabetic rats (Figure 2A) . These findings indicate that insulin prevented the glucose-dependent increase in the expression of these selected cytokines and ECM genes.
To further analyze the contribution of CTGF in regulating ECM molecules, we developed a siRNA-approach to inhibit CTGF. We tested if inhibition of CTGF by siRNA affected the expression of laminin β1, fibronectin 1, collagen IVα3, and VEGF. In addition, we also tested the effect of the treatment on glial fibrillary acidic protein (GFAP), an intermediate filament protein that increases in the retina during DR [34,35],
We first used an in vitro system to determine the specificity of three siRNAs in downregulating CTGF levels in a rat cell line. Since we previously showed that TGF-β induces a twofold increase in CTGF mRNA and a significant increase in the CTGF protein in Rat-2 fibroblasts , we tested whether the induction of CTGF was inhibited by any of the three CTGF siRNAs (siRNA I–III) alone or in combination. Previous studies showed that CTGF protein levels in Rat-2 cells were undetectable in the absence of TGF-β . Real-time PCR showed that siRNA I and siRNA III decreased TGF-β induced CTGF mRNA by 75% and 86% (p<0.05), respectively (Figure 5A). In contrast, siRNA II had no effect on reducing CTGF mRNA (data not shown). Western blot analysis using siRNA I and siRNA III revealed that CTGF protein decreased by 49% and 46%, respectively (Figure 5B,C). The combination of siRNA I and III did not result in further inhibition of CTGF (data not shown). siRNA I was chosen for the in vivo experiments because it gave the greatest decrease in CTGF protein.
Then we sought to determine whether the siRNA reached all layers of the retina. Animals were given a single intravitreal injection of Cy3-labeled scrambled siRNA, and the eyes were harvested 3 days after the injection, sectioned, and viewed using confocal microscopy. Labeled siRNA was distributed throughout the retina from the ganglion cell to the photoreceptor layers (Figure 6A,B,D). The contralateral eyes were injected with unlabeled siRNA to test whether the light emissions observed in the eyes injected with labeled siRNA was due to autofluorescence produced by the siRNA. Retinas of rats that received unlabeled siRNA did not show any detectable fluorescence (Figure 6C). The distribution of labeled siRNA throughout the retina confirms previous reports by Shen et al. .
To determine whether the siRNA treatment had a beneficial effect on the retinas of diabetic rats, 12-week hyperglycemic rats were given a single intravitreal injection of CTGF siRNA in one eye (the experimental retina), while the contralateral eye was injected with scrambled siRNA (the control retina). Three days later, the retinas were dissected and processed for mRNA and protein analysis. Administering CTGF siRNA induced a decrease in CTGF (33%, p<0.05), collagen IVα3 (71%, p<0.05), and laminin β1 (63%, p<0.05) mRNA levels (Figure 7A). Levels of GFAP mRNA decreased by 44% (p<0.05) in the CTGF siRNA–treated retina (Figure 7A). Importantly, the level of CTGF protein was 54% lower (p<0.05) in the experimental retinas compared to the control retinas (Figure 7B-C). In contrast, administering CTGF siRNA did not affect VEGF or fibronectin levels, which remained similar in the experimental and control retinas (Figure 7A). The effect of the siRNA treatment decreased with time since the CTGF mRNA levels were similar in the experimental and control retinas 10 days after CTGF siRNA was injected (Figure 7D).
Although insulin therapy aids in preventing DR, since insulin stabilizes endothelial barrier function  and decreases microvascular leakage , the role of insulin in regulating ECM molecules is not well defined. In this study, our first goal was to determine whether CTGF, a profibrotic molecule induced by high glucose [5,13], was downregulated with insulin therapy and whether this decrease also affected extracellular matrix components proposed to be controlled by CTGF . We found that the elevated levels of CTGF mRNA and protein induced by hyperglycemia were prevented by exogenous insulin treatment. Moreover, insulin therapy also inhibited the upregulation of several components of the extracellular matrix such as laminin β1, collagen IVα3, and fibronectin, and of GFAP and VEGF.
Importantly, we determined that Müller cells in the diabetic retina immunostained with a specific antibody to CTGF. Although CTGF is a secreted protein, it is not surprising that it is localized within the cytoplasm of Müller cells. Other secreted proteins, such as hormones, are also localized to the cytoplasm of the cells that synthesize them. In contrast to our findings, previous immunohistochemical studies reported the expression of CTGF by cells of the ganglion cell and inner plexiform layers in rodents [5,15] and in microglial cells and pericytes in humans . The discrepancy between our results and that of others could be due to the different histological techniques employed in the analysis and/or to the specificity of the antibodies used. In situ hybridization studies reported the expression of CTGF mRNA by structures located in the ganglion cell layer  and proposed that it was expressed by the end feet of Müller cells . Although in situ hybridization identifies the site of mRNA expression, identifying the cell type that is labeled is often difficult. For that reason, we used immunohistochemistry to visualize CTGF. Our results are in agreement with the cell type proposed by that group to synthesize CTGF. The antibody did not stain CTGF bound to the cell membrane of cells that respond to the action of this cytokine. Although a specific CTGF receptor has not yet been identified, CTGF appears to perform many of its functions through integrins, heparin sulfate–containing proteoglycans, and the low-density lipoprotein receptor–related protein . Although CTGF probably binds to any or all of these receptors, its levels at the cell membrane are probably below the sensitivity of the techniques used.
Müller cells become activated by high glucose levels and upregulate the expression of GFAP, and of VEGF and other angiogenic cytokines [35,40]. The localization of CTGF to Müller cells has important clinical applications since these cells participate in maintaining the homeostasis of the retinal extracellular milieu and protect neurons via a release of neurotrophic factors; disturbance of these cells could lead to retinal dysfunction .
Although insulin therapy downregulated the level of expression of CTGF and ECM molecules, oscillations in blood glucose occur even in the presence of tight glycemic control , and these changes could affect retinal function even in well controlled patients . To circumvent possible harmful effects of blood glucose oscillations, we sought to develop a siRNA approach for short-term inhibition of CTGF. Our goal was to determine whether a reduction in CTGF expression in diabetic rats affected the activity of genes regulating the synthesis of selected ECM molecules. We found that the siRNA treatment specifically decreased CTGF expression in vitro and in vivo. In vivo, siRNA molecules labeled with Cy3 were found in all layers of the retina. This observation suggests that the injected molecule reaches all retinal cells but affects only the level of CTGF expression by Müller cells. Since other retinal cell types do not express CTGF, their gene expression is not likely to be affected due to the exquisite specificity of the siRNA approach.
We demonstrated that siRNA treatment decreased CTGF mRNA and protein. This effect is specific, because the treatment downregulated the 36–38 kDa form of CTGF, the primary form of the cytokine . In contrast to our finding, a recent study using a similar approach reported a decrease in a 55 kDa protein probed with a CTGF antibody and no change in the 36–38 kDa forms . The identity of the 55 kDa protein is unknown. Moreover, the specificity of the siRNA treatment in Yang et al.’s report is unclear since the synthetic oligonucleotides used in that report also decreased VEGF . In contrast, in our study the CTGF siRNA did not affect VEGF mRNA levels, supporting multiple reports indicating that VEGF is upstream of CTGF [14,15,45].
Our results reveal that the CTGF-specific siRNA resulted in a decrease in laminin β1 and collagen IVα3 mRNA levels, indicating that these two genes are CTGF targets. In contrast, inhibition of CTGF did not change fibronectin mRNA levels. This result was unexpected because studies in other tissues reported that CTGF regulates fibronectin expression [19,46]. This discrepancy could be due to differences in the half-life of fibronectin mRNA in different cell types. We also found that CTGF siRNA reduced GFAP expression, indicating that CTGF regulates the level of expression not only of extracellular molecules but also genes coding for intracellular proteins. We did not examine the protein levels of ECM molecules following the siRNA treatment. The short duration of action of the siRNA and the relatively long half-life of extracellular matrix proteins  suggest that, in our studies, the siRNA treatment did not affect protein levels.
Although the siRNA experiments support a role for CTGF in regulating ECM molecules, the effect of the injected siRNA in diabetic rats lasted for only 3 days since the experimental and contralateral control retinas expressed similar levels of CTGF mRNA 10 days after the injection. Other studies also reported a short duration of siRNA treatments [36,48]. Therefore, although our findings support the use of an siRNA approach to complement insulin therapy, future studies should seek to circumvent its limitations. One limitation of siRNA treatment is the ability of siRNA to nonspecifically bind to toll-like receptor 3, resulting in an off-target antiangiogenic response . In addition, the approach requires the development of chemically modified siRNA molecules that will stabilize and extend the duration of the treatment when combined with appropriate transfection reagents. In conclusion, our results clearly demonstrate that CTGF regulates the level of expression of ECM molecules as well as GFAP, a specific glial cell filament.
There are no potential conflicts of interest relevant to this article. Parts of this study were presented in abstract form at the American Diabetes Association scientific sessions 2010, Orlando, Florida, June 25–29. The authors wish to thank Dr. John Danias (SUNY Downstate Medical Center, Brooklyn, NY) for critically reading the manuscript. This work was supported by a pilot project grant from the Juvenile Diabetes Research Foundation International.