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Originally published In Press as doi:10.1167/iovs.09-3460 on April 22, 2009
 (Investigative Ophthalmology and Visual Science. 2009;50:3542-3552.)
© 2009 by The Association for Research in Vision and Ophthalmology, Inc.
doi:10.1167/iovs.09-3460
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Inhibition of Human Scleral Fibroblast Cell Attachment to Collagen Type I by TGFBIp

Lilian Shelton and Jody A. Summers Rada

From the Department of Cell Biology, University of Oklahoma Health Science Center, Oklahoma City, Oklahoma.


   Abstract
Top
 Abstract
Methods
 Results
 Discussion
 References
 
PURPOSE. Transforming growth factor β–induced protein (TGFBIp; 68 kDa) is a secreted extracellular matrix (ECM) protein that has been demonstrated to regulate cell attachment in a variety of cell types. The sclera synthesizes and secretes TGFBIp, which may function to facilitate scleral ECM remodeling events associated with myopia development. Here the authors report that human scleral fibroblasts (HSFs) express TGFBI and that its protein product, TGFBIp, mediates an effect on cell attachment.

METHODS. TGFBI/TGFBIp expression was evaluated by RT-PCR and immunoblot of HSF lysates and culture supernatants. The effect of rTGFBIp (50 µg/mL) on cell attachment to collagen type I was determined with the use of fluid-phase cell attachment assays in HSFs, human foreskin fibroblasts (HFFs), and human corneal stroma fibroblasts (HCFs). Binding assays using biotinylated rTGFBIp were used to assess TGFBIp binding to the HSF surface. Flow cytometry and immunocytochemistry were used to determine both {alpha}vβ3 and {alpha}vβ5 expression and localization to the HSF cell surface.

RESULTS. HSFs expressed TGFBI and secreted TGFBIp (~833 ng/h). rTGFBIp significantly decreased (25 µg/mL; P ≤ 0.05) HSF attachment to collagen type I, whereas rTGFBIp did not significantly affect cell attachment of HFFs (P = 0.50) or HCFs (P = 0.24) to collagen compared with BSA. Integrins {alpha}vβ3 and {alpha}vβ5 were detected on the cell surface, and both anti-{alpha}vβ3 and anti-{alpha}vβ5 functionally blocked rTGFBIp binding to HSFs.

CONCLUSIONS. TGFBIp plays an inhibitory role in HSF attachment to collagen type I in vitro through interactions with {alpha}vβ3 and {alpha}vβ5 integrin receptors. These results suggest that TGFBIp may modulate scleral cell–matrix interactions in vivo, thereby affecting scleral viscoelasticity.

The mammalian sclera provides structural support for the delicate inner ocular tissues and defines the size, shape, and refractive status of the eye. The sclera is a dense connective tissue consisting largely of extracellular matrix (ECM) containing collagen types I and III (Zorn N, et al. IOVS 1992;33:ARVO Abstract S1053; Norton TT, et al. IOVS 1995;36:ARVO Abstract S760)1 2 3 and lesser amounts of collagens IV, V, VI, VIII, XII, and XIII (Zorn N, et al. IOVS 1992;33:ARVO Abstract S1053; Norton TT, et al. IOVS 1995;36:ARVO Abstract S760),1 2 3 4 5 6 7 proteoglycans (Johnson JM, et al. IOVS 2002;43:ARVO E-Abstract 1100),8 9 10 11 12 and noncollagenous glycoproteins.13 14 The scleral ECM is organized into irregularly arranged collagenous lamellae that are continuous with the highly ordered collagenous lamellae of the cornea at the corneal limbus. Located between the collagenous lamellae of the sclera are scleral fibroblasts that are responsible for the synthesis and turnover of the scleral ECM.15

Myopia is a common abnormal visual condition characterized by a negative refractive error that occurs when the eye is too long for its focal length. In humans, this ocular elongation is associated with significant scleral thinning and alterations in collagen fibril density and morphology at the posterior pole of the eye.16 17 18 Mammalian models of myopia have also demonstrated scleral thinning as well as changes in gene expression and protein synthesis during the development of myopia.15 19 20 21 22 23 24 25 26 More specifically, myopia development in mammals is associated with a decreased rate of proteoglycan synthesis,20 24 27 28 decreased collagen fibril diameter and synthesis,3 18 21 29 and increased matrix metalloproteinase (MMP)-2 activity.21 30 31 32 Although the events leading to myopia development are not clear, these biochemical changes in the scleral extracellular matrix have been associated with alterations in the biomechanical properties of the sclera and are thought to be responsible for the increased rate of ocular elongation and myopia development.33 34 35

Of much interest are the molecular mechanisms that regulate scleral cell–matrix interactions under normal ocular growth conditions and under conditions of increased ocular elongation and myopia development. Observations in animal models strongly suggest that local factors within the eye play important roles in the regulation of ocular growth.19 36 37 38 39 40 Furthermore, scleral proteoglycan synthesis has been shown to be regulated in part by the involvement of the underlying vascular layer of the eye, the choroid.41 42 43 These studies suggest that the eye is not dependent on the brain for visually guided growth regulation but, rather, is dependent on a cascade of chemical events extending from the retina to the sclera that act to control vitreous chamber elongation.

Recently, microarray analyses were used to identify genes differentially expressed in choroid/RPEs in eyes of young marmosets (Callithrix jacchus) during varying ocular growth states.44 The transforming growth factor β-inducible gene-h3 (TGFBI; also known as BIGH3, βIGH3) was shown to be significantly increased in the choroid/RPE of eyes compensating for –5 D lenses (relative myopia) compared with contralateral +5 D lens–treated eyes (relative hyperopia). Additionally, expression of the TGFBI gene product TGFBIp (also known as BIGH3, βIG-H3, and keratoepithelin)45 46 was identified in marmoset and human cornea and choroid/RPE and was also present at high levels in the sclera.44

To date, several studies have suggested that TGFBIp plays a functional role in cell adhesion, migration, proliferation, wound healing, inflammation, tumorigenesis, angiogenesis, nephropathies, and corneal dystrophy.47 Until now, TGFBI/TGFBIp expression and its possible functional role(s) in the sclera have not been studied. Therefore, in the present study, in vitro analyses using primary human scleral fibroblasts (HSFs) were undertaken to evaluate the scleral expression of TGFBI/TGFBIp and to determine its role in mediating scleral fibroblast attachment to collagen type I. The results of these studies demonstrate that TGFBIp selectively and specifically inhibits attachment of HSFs to collagen type I, most likely through interactions with {alpha}vβ3 and {alpha}vβ5 integrin receptors located on the HSF cell surface. These results may provide insight into the role of TGFBIp in scleral remodeling events required for normal ocular growth and during the development of myopia.


   Methods
Top
 Abstract
 Methods
Results
 Discussion
 References
 
Cell Culture
Primary HSFs were isolated from explants of human donor sclera as previously described and stored in liquid nitrogen until use.48 49 Primary human corneal fibroblasts (HCFs) were isolated from stromal explants from the central regions of human donor corneas as previously described and stored in liquid nitrogen until use.50 HSFs passages 4 to 6 (P4–6) and HCFs P6–9 were cultured on 100-mm plates containing Dulbecco modified Eagle medium (DMEM), penicillin (100 U/mL)-streptomycin (100 µg/mL), amphotericin B (0.0025 µg/mL; 1x a/a [Invitrogen Corp., Carlsbad, CA]), and 15% fetal bovine serum (FBS) at 37°C with 95% air/5% CO2. Human foreskin fibroblasts (HFFs) P3–6 were obtained from American Type Culture Collection (ATCC, Manassas, VA) and were cultured in Iscove modified Eagle medium (IMEM; ATCC) containing 1x a/a and 10% FBS at 37°C with 95% air/5% CO2. HSF-conditioned medium was obtained from confluent cultures by replacing the culture media with serum-limiting media (DMEM containing 1x a/a and 0.05% FBS) and incubating the media for 48 hours at 37°C in 95% air/5% CO2. For cell attachment assays (see below), culture media were removed from confluent cultures, and cells were rinsed once and incubated in 0.53 mM EDTA in Hanks balanced salt solution (HBSS; Sigma-Aldrich, St. Louis, MO) at 37°C for 10 minutes After incubation in 0.53 mM EDTA, cells were detached by gentle pipetting, centrifuged, and resuspended in DMEM containing 1x a/a before counting with a hemocytometer.

RNA Isolation and Cell Lysate Preparation
After the 48-hour incubation, the conditioned media were collected, and either RNA was isolated or cell lysates were obtained from the HSF cell layers. Total RNA was isolated from HSF monolayers using reagent (Trizol; Invitrogen) according to the standard protocol, as previously described.44 Isolation of whole cell extracts was performed using a commercial mammalian cell lysis buffer (M-PER; Pierce Chemical, Rockville, IL), protease inhibitor cocktail set 1 (EMD Biosciences, San Diego, CA), phosphatase inhibitor cocktail 2 (Sigma Chemical, St. Louis, MO), and NaCl. Protease inhibitor cocktail set 1 contained five protease inhibitors that inhibited a broad range of proteases (500 µM 4-(2-aminoethyl)benzenesulfonylfluoride-hydrochloride, 150 nM aprotinin, 1 µM E-64 protease inhibitor, 0.5 mM EDTA-disodium, 1 µM leupeptin-hemisulfate), and phosphatase inhibitor cocktail 2 contained a proprietary mixture of inhibitors that inhibited acid and alkaline phosphatases and tyrosine protein phosphatases (sodium orthovanadate, sodium molybdate, sodium tartrate, imidazole). The lysis buffer was prepared by diluting protease inhibitor cocktail set 1 (1:100) and phosphatase inhibitor cocktail set 2 (1:100) in mammalian cell lysis buffer (4.6 mL; M-PER; Pierce Chemical) containing 150 mM NaCl. Briefly, the cells were washed with ice-cold PBS for 1 minute before the addition of lysis buffer (200 µL/plate), then scraped with a rubber policeman and collected. After incubation (15 minutes) on ice and centrifugation (12,000g) for 5 minutes, the supernatant was collected and stored at –20°C until use.

Reverse Transcription–Polymerase Chain Reaction
cDNA was synthesized from total RNA using MuLV reverse transcriptase together with random hexamers, dNTPs in the presence of PCR buffer, 25 mM MgCl2, and RNase inhibitor (GeneAmp kit; Applied Biosystems, Foster City, CA) as previously described.44 48 Primers specific for human TGFBI and cyclophilin A (peptidylprolyl isomerase A [PPIA]) were designed and purchased using BLAST, Primer3 (http://frodo.wi.mit.edu/cgi-bin/primer3/primer3_www.cgi) and Sigma-Genosys (St. Louis, MO), respectively, and diluted to 15 µM in RNase-free water as previously described.44 PPIA served as a positive control in this study because it has been routinely used as a housekeeping gene to normalize for gene expression differences and has previously been shown to consistently generate high-quality PCR products with a high efficiency while showing no significant differences in steady state mRNA levels in the choroid/RPE of minus lens-treated eyes (undergoing relative myopia development) compared with that of plus lens-treated eyes (undergoing relative hyperopia development) in marmosets.44

Each reaction underwent 35 amplification cycles consisting of denaturation at 94°C for 30 seconds, annealing for 30 seconds at 60°C, and extension for 30 seconds at 72°C using a thermal cycler (DNA thermal cycler 480; Perkin Elmer, Norwalk, CT). To control for genomic DNA contamination, reverse transcriptase was omitted from some samples before PCR amplification. Aliquots of each PCR reaction were electrophoresed on a 1.5% agarose gel containing ethidium bromide (0.5 µg/mL) and visualized on an imager (Chemigenius; Syngene USA, Frederick, MD).

Western Blot Analysis
After 48 hours of incubation in DMEM + 0.05% FBS, conditioned medium was collected from HSF cell cultures, and cell lysates were dried under a vacuum in a concentrator (Speed-Vac; Savant, Holbrook, NY) and reconstituted in one-tenth of the original volume with RNase-free water to concentrate the intracellular TGFBIp protein. Scleral cell lysates and aliquots of conditioned medium were directly applied to 10% SDS-PAGE gels (Bis-Tris Gel NuPAGE; Invitrogen). Gel samples were electrophoresed under reducing conditions and electroblotted onto a nitrocellulose membrane using an electro-transfer unit (XCELL Sureback Electrophoresis Cell; Invitrogen) according to the manufacturer’s instructions. Blots were blocked with PBS containing 0.1% Tween-20 and casein-based blocking agent (0.2% I-Block; Tropix, Bedford, MA) for 1 hour and then probed with anti–human TGFBIp (1:500; R&D Systems, Minneapolis, MN) or mouse monoclonal {alpha}-tubulin (1:10,000; Abcam, Cambridge, MA) antibodies overnight at 4°C. Anti–human TGFBIp is a polyclonal antibody that was produced in goats immunized with purified, NS0-derived (mouse myeloma cell line), mature recombinant human TGFBIp protein (Gly 24-His 683).45 The specific epitope(s) this antibody recognizes has not been characterized but has been used in a previous study to recognize a 68-kDa band in primate ocular tissues.44 Immunoblots were then washed three times for 10 minutes with PBS containing 0.05% Tween-20 and incubated with rabbit anti–goat IgG (whole molecule) conjugated to alkaline phosphatase or goat anti–mouse IgG (whole molecule) conjugated to alkaline phosphatase secondary antibodies (1:1000; Sigma) for 1 hour at room temperature. After incubation with secondary antibody, blots were washed, incubated (CDP-Star Ready-to-Use with Nitro-BlockII; Tropix, Bedford, MA) for 5 minutes, and then imaged (Chemigenius; Syngene USA) or exposed to film. In some cases, protein-blocking experiments were carried out in which anti–human TGFBIp was preincubated with an equimolar amount (1 µM) of human recombinant TGFBIp (rTGFBIp; R&D Systems) for 1 hour at room temperature before use in Western blots.

Cell Attachment Assay
Ninety-six-well plates were precoated with 10 µg/mL rat tail collagen type I (100 µL/well; Sigma-Aldrich) and incubated overnight at 4°C. After removing excess liquid from the wells, the plate was sterilized in ultraviolet light under a culture hood overnight, and the wells were rinsed with PBS. HSFs were resuspended in DMEM/1x a/a containing 0.5% FBS at a concentration of 2000 cells/200 µL containing 0 to 50 µg/mL bovine serum albumin (BSA; Sigma), fibronectin (FN; Sigma) or rTGFBIp. For antibody-blocking experiments, an equimolar amount of anti-TGFBIp antibody (50 µg/mL; R&D Systems) was preincubated with rTGFBIp (25 µg/mL; R&D Systems) for 1 hour at room temperature before cells were added. Cells were immediately seeded in triplicate (2000 cells/well) to collagen-coated plates and permitted to attach for 45 minutes at 37°C (95% air containing 5% CO2) before gently rinsing off the unattached cells twice with PBS. Finally, toluidine blue (150 µL; 0.5% toluidine blue stain in 4% paraformaldehyde [wt/vol]) was added to each well for 5 minutes at room temperature and removed, and the wells were rinsed three times with ultrapure water (Milli-Q; Millipore, Temecula, CA) before solubilization with 1% SDS (250 µL). Cell numbers were determined by reading absorbance at 595 nm using a plate reader (Bio-Rad, Hercules, CA) and comparing that to a standard curve prepared from 0 to 10,000 cells/well.

TGFBIp Binding Assay
rTGFBIp (R&D Systems) was biotinylated with a biotinylation kit (EZ-Link Micro Sulfo-NHS; Pierce, Rockford, IL) according to the manufacturer’s instructions. Briefly, 11 mM sulfo-NHS-biotin in PBS was added in a 50-fold molar excess to rTGFBIp (6 µL; 11 mM Sulfo-NHS-biotin in PBS/per 500 µL rTGFBIp) and incubated while rotating at room temperature for 1 hour. During the incubation, a desalt spin column (Zeba; Pierce) was prepared by centrifugation at 1000g for 2 minutes (Sorvall RT 6000D; DuPont, Hoffman Estates, IL) to remove the storage buffer and equilibrate the column (three washes with 1 mL PBS). After the 1-hour incubation, the protein-biotin mixture was placed onto the column and allowed to absorb into the resin before centrifugation at 1000g for 2 minutes. The flow through, consisting of purified biotinylated rTGFBIp, was collected and stored at –20°C until use. The bicinchoninic acid (BCA) protein assay (Pierce Chemical) was used to determine the concentration of the biotinylated rTGFBIp spectrophotometer (NanoDrop ND-1000; NanoDrop Technologies, Wilmington, DE) as previously described.44

Binding assays were performed as described previously with slight modification.51 52 53 HSFs were suspended in serum-free medium (DMEM + 1x a/a) at a density of 1 x 105 cells/mL, centrifuged at 1000 rpm for 5 minutes at 4°C, washed in ice-cold PBS, recentrifuged at 1000 rpm for 5 minutes, and reconstituted in serum-free medium containing biotinylated rTGFBIp (0–50 µg/mL) and incubated at 4°C for 5 hours with rotation. Next, the cells were washed three times with ice-cold PBS and were lysed by the addition of 100 µL cell lysis buffer. Equal amounts (10 µL) of protein from each sample were separated on a 10% SDS-PAGE gel and then transferred to a nitrocellulose membrane. Biotinylated rTGFBIp was visualized by incubation of membranes with streptavidin conjugated to alkaline phosphatase (1:3000; Sigma). Biotinylated and nonbiotinylated rTGFBIp were also visualized by incubating the blots with anti-TGFBIp antibody (1:500) overnight at 4°C followed by incubation with anti–goat IgG conjugated to alkaline phosphatase and imaged with CDP-Star chemiluminescent substrate. After detection of biotinylated rTGFBIp, blots were stripped (Restore Plus Western Blot Stripping Buffer; Pierce) according to the manufacturer’s protocol and were reprobed with {alpha}-tubulin antibody (1:10,000) for an internal control. For some experiments, 1 mL HSF cell suspension was preincubated with anti–mouse {alpha}vβ3 or anti–mouse {alpha}vβ5 integrin antibody (final concentration, 0–10 µg/mL; Millipore) for 1 hour at 4°C with rotation before washing three times with ice-cold PBS and incubation with biotinylated rTGFBIp.

Additionally, competitive displacement experiments were carried out in which HSFs were incubated with nonbiotinylated rTGFBIp (0–50 µg/mL) in serum-free medium for 3 hours at 4°C, washed in ice-cold PBS, and incubated with 10 µg/mL biotinylated rTGFBIp for 3 hours at 4°C. Cells were washed again and lysed, and biotinylated and total rTGFBIp were detected by Western blot analysis using streptavidin and anti-TGFBIp, respectively, as described.

Flow Cytometric Analysis
To confirm the expression of a specific integrin(s) on the surfaces of HSFs, fluorescence-activated cell sorter analyses were performed. HSFs were grown to confluence in serum-containing medium and detached from plates by treatment with HBSS containing 0.05% EDTA, as described previously. The cells were rinsed twice in wash buffer (PBS containing 0.1% BSA), resuspended in wash buffer at a concentration of 1 x 105 cells/mL, and incubated for 1 hour at 4°C with 4 µg/mL of monoclonal mouse anti–integrin {alpha}vβ3 (clone LM609) or anti-{alpha}vβ5 (clone P1F6) antibodies (Millipore). Cells were pelleted by centrifugation at 1000 rpm for 5 minutes, supernatants were removed, and cell pellets were rinsed three times with wash buffer. Cells were then incubated in the dark for 1 hour at 4°C with 10 µg/mL Alexa Fluor 568 rabbit anti–mouse IgG (Molecular Probes, Eugene, OR). Cells were pelleted, washed again, and analyzed on a flow cytometry system (FACSCalibur; Becton Dickinson, San Jose, CA).

Immunofluorescence
HSFs were grown in 100-mm dishes in serum-containing medium, detached, and seeded onto 12-mm round coverslips in a 24-well culture dish in serum-containing medium (Corning Incorporated, Corning, NY). After 24 hours of incubation at 37°C, the culture media were aspirated, and the coverslips were washed twice with PBS containing 0.5 mM CaCl2 and MgCl2 (PBS++) to remove unattached cells. Cells were then fixed in 4% paraformaldehyde in wash buffer for 5 minutes at room temperature, followed by a 15-minute incubation in 4% paraformaldehyde on ice before washing 3x for 5 minutes with wash buffer. Coverslips containing fixed cells were incubated with nonimmune mouse IgG, anti-TGFBIp, anti-{alpha}vβ3 or anti-{alpha}vβ5 antibodies (1:100 dilution in PBS++ containing 0.1% FBS) for 1 hour at room temperature. After washing, the coverslips were incubated with the appropriate secondary antibody conjugated to AlexaFluor 488 or AlexaFluor 568 (1:200 dilution in PBS++ containing 0.1% FBS) in the dark for 1 hour at room temperature. After washing six times for 10 minutes with PBS++, the coverslips were rinsed in ultrapure water mounted to slides using antifade reagent containing DAPI (ProLong Gold; Invitrogen). Cells were then viewed under a confocal laser scanning microscope (Fluoview FV1000; Olympus America Inc., Melville, NY).

Statistical Analysis
Statistical comparisons were made using the Student’s t-test for unmatched pairs or one-way ANOVA with Bonferroni adjustments (GraphPad Prism, version 4.03 for Windows; GraphPad Software, San Diego, CA). Nonlinear regression analysis with the sigmoidal dose-response equation for variable slopes was used to determine the required concentration to reach 50% inhibition (IC50).


   Results
Top
 Abstract
 Methods
 Results
Discussion
 References
 
TGFBI/TGFBIp Expression by HSFs
TGFBI gene expression by HSFs was confirmed by RT-PCR using human primers specific to TGFBI together with the housekeeping gene PPIA, which served as the positive control. After electrophoresis on a 1.5% agarose gel, single bands at 373 bp and 300 bp could be detected for TGFBI and PPIA, respectively (Fig. 1A) . No bands were observed when reverse transcriptase was omitted from the PCR reactions (data not shown), indicating that PCR amplicons were not the result of DNA contamination. TGFBIp expression in scleral fibroblast cell lysates and in culture supernatants was evaluated by Western blot analysis. A 68-kDa band was observed in the conditioned media (Fig. 1B ; 1x media, top). A faint 68-kDa band (Fig. 1B ; 10x cell lysates, top) could be identified on 10x concentrated cell lysates, and no bands were detected in culture media in the absence of HSFs (Fig. 1B ; top; DMEM + 0.05% FBS). All bands were abolished when rTGFBIp was preincubated with an equimolar amount (1 µM) of the primary anti-TGFBIp antibody, thereby confirming the specificity of the antibody used (Fig. 1B , middle). Comparison of TGFBIp in scleral fibroblast culture supernatants (1x conditioned media) with a standard curve prepared from rTGFBIp (0.5–5.0 µg) indicated that HSFs secreted abundant levels of TGFBIp (~4 µg/mL per 48 hours; ~833 ng/h; Fig. 1C ).


Figure 1
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  		FIGURE 1. TGFBI/TGFBIp expression in 48-hour serum-starved HSFs. (A) RT-PCR amplification of TGFBI (373 bp) and PPIA (300 bp) from HSFs. (B) Western blot of HSF cell lysates (10x) and media (1x) probed with anti-TGFBIp (top). Human recombinant TGFBIp (rTGFBIp, 40 ng) and DMEM containing 0.05% FBS served as the positive and negative control, respectively. Preincubation of anti-TGFBIp with an equimolar amount of rTGFBIp (1 µM) for 1 hour at room temperature abolished all immunopositive bands, confirming the specificity of the antibody (rTGFBIp block, middle). Total protein loaded in each lane was visualized by Coomassie blue (bottom). (C) Indicated quantities of rTGFBIp were compared with several dilutions of 48-hour HSF conditioned medium (10 µL/lane).

 
TGFBIp Modulates HSF Adhesion to Collagen
To assess the effects of TGFBIp on cell adhesion to collagen type I, primary HSFs were plated on collagen-coated, 96-well plates in the presence of BSA, FN, rTGFBIp, and anti-TGFBIp antibody (Fig. 2) . rTGFBIp significantly inhibited HSF attachment at concentrations of 25 µg/mL (–32% ± 12.6%; P < 0.05) and 50 µg/mL (–47% ± 2.1%; P < 0.01) in a dose-dependent manner compared with BSA alone (Fig. 2A) . HSFs treated with antibody-neutralized rTGFBIp (25 µg/mL rTGFBIp + 50 µg/mL anti-TGFBIp) showed a significant increase in attachment to collagen compared with cells treated with rTGFBIp alone (+34% ± 5.0%; P < 0.01) and no significant difference compared with BSA (+9% ± 7.4%; P = 0.29). HSF attachment to collagen in the presence of anti-TGFBIp alone (50 µg/mL) was similar to cell attachment to BSA-treated, collagen-coated wells (+7% ± 2.1%; P = 0.20).


Figure 2
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  		FIGURE 2. Inhibitory role of TGFBIp on cell attachment is specific to HSFs. (A) HSF attachment to collagen type I in the presence of BSA, FN, or rTGFBIp (1–50 µg/mL). (B) HSF attachment to collagen type I in the presence of BSA, FN, rTGFBIp (25 µg/mL) with or without anti-TGFBIp (50 µg/mL). (C) Attachment of HFFs to collagen type I in the presence of BSA, FN, rTGFBIp (25 µg/mL) with or without anti-TGFBIp (50 µg/mL). (D) Attachment of HCFs to collagen type I in the presence of BSA, FN, rTGFBIp (25 µg/mL) with or without anti-TGFBIp (50 µg/mL). Micrograph of HCFs before harvesting for cell attachment assays demonstrating a distinct fibroblast phenotype (inset). Data are expressed as the mean ± SEM for three experiments conducted in triplicate. **P < 0.01. NS, not significant using ANOVA with Bonferroni post-hoc correction.

 
The effect of TGFBIp on cell adhesion was also assessed using HFFs (P = 0.50; Fig. 2C ); however, treatment with rTGFBIp together with equimolar amounts of anti-TGFBIp showed a significant decrease in attachment compared with BSA (–28% ± 3.8%; P < 0.01). Similarly, rTGFBIp did not appear to affect HCF attachment to collagen type I compared with BSA (+37% ± 23.7%; P = 0.24; Fig. 2D ); in contrast to HFFs, treatment of HCFs with antibody-neutralized rTGFBIp did not appear to affect attachment compared with BSA (–22% ± 22.7%; P = 0.51). These results demonstrate that TGFBIp inhibits HSF adhesion to collagen type I but does not affect the adhesion of HFF or HCF to collagen. Previous studies have demonstrated that when corneal keratocytes are grown in the presence of serum, they take on a fibroblast phenotype, actively proliferate, and do not express the keratocyte-specific protein keratocan.50 54 55 56 Based on our growth conditions and the phenotype of the cells (Fig. 2D , inset), the corneal cells used in these cell attachment studies most closely resemble corneal fibroblasts rather than corneal keratocytes or myofibroblasts.

TGFBIp Binds to the Surfaces of HSFs
Biotinylation of rTGFBIp (100 ng) did not alter the expected 68-kDa band compared with rTGFBIp (100 ng) when probed with streptavidin conjugated to alkaline phosphatase (Fig. 3A) . To determine whether TGFBIp directly binds to the surfaces of HSFs, HSFs were incubated with biotinylated rTGFBIp (0–50 µg/mL), and specific binding was determined by visualizing biotinylated rTGFBIp with streptavidin-alkaline phosphatase with Western blot analysis (Fig. 3B) . Biotinylated rTGFBIp was observed as a single band migrating at 68 kDa (arrowhead). In addition, a biotinylated higher molecular weight band of 136 to 140 kDa was detected on blots, most likely because of nonspecific binding of streptavidin to a protein(s) in the cell lysates. Binding of biotinylated rTGFBIp to HSFs was saturable at concentrations ≥0.37 nM (25 µg/mL; Bmax), and 50% maximal binding was achieved at 0.15 nM (10 µg/mL).


Figure 3
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  		FIGURE 3. TGFBIp binds to the surfaces of HSFs in a dose-dependent manner. (A) Western blot of both rTGFBIp (100 ng) and biotinylated rTGFBIp (100 ng). Blots were probed with streptavidin conjugated to alkaline phosphatase, then stripped and reprobed with anti-TGFBIp. (B) Western blot of HSF lysates incubated with increasing concentrations of biotinylated rTGFBIp (0–50 µg/mL) probed with streptavidin conjugated to alkaline phosphatase, and histogram of band densities. Binding of biotinylated rTGFBIp to HSFs was saturable at ≥0.37 nM (25 µg/mL; Bmax).

 
To investigate the specificity of TGFBIp displacement to the HSF cell surface, competitive binding assays were performed by assessing biotinylated 0.15 nM rTGFBIp (10 µg/mL) binding to HSFs in the presence of increasing amounts of nonbiotinylated competitor rTGFBIp (0–0.74 nM [50 µg/mL]; Fig. 4A ). The concentration of biotinylated rTGFBIp used in competitive displacement assays was determined based on the estimated Km for rTGFBIp binding (0.185 nM). Analysis of band intensities after the competitive displacement assays indicated that the concentration of rTGFBIp required for 50% inhibition (IC50) of binding to HSFs in vitro was 0.03 nM (Fig. 4B) . Ideally, half the data points on the IC50 curve are above the IC50 value and half are below the IC50 value; unfortunately, however, this did not occur in our experiments. Therefore, additional points (inhibitor concentrations) should be included for a more accurate IC50 determination. However, based on the criterion that the maximum inhibition be greater than 50%, we elected to include these results as shown.


Figure 4
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  		FIGURE 4. Competitive displacement of biotinylated rTGFBIp with nonbiotinylated rTGFBIp. (A) Representative Western blot from three independent experiments in duplicate of cell lysates from HSFs incubated with soluble biotinylated rTGFBIp (0.15 nM), washed with PBS, then incubated with increasing amounts of nonbiotinylated rTGFBIp competitor (0–0.74 nM) probed with anti-TGFBIp and streptavidin conjugated to alkaline phosphatase. Note the reduced biotinylated rTGFBIp binding in the presence of the competitor. Arrowhead: position of the 68-kDa band. (B) Competitive inhibition curve for specific binding of biotinylated rTGFBIp by increasing concentrations of nonbiotinylated rTGFBIp. The 50% inhibition concentration (log IC50) was calculated to be –1.54 nM (IC50 = 0.03 nM). Data are expressed as band intensity of biotinylated rTGFBIp relative to {alpha}-tubulin, and were fit into an IC50 equation. For the loading control, all blots were stripped and reprobed with {alpha}-tubulin antibody.

 
TGFBIp Binds to Specific Integrins on HSFs
Flow cytometry was performed using monoclonal antibodies specific for {alpha}vβ3and {alpha}vβ5 integrins. Compared with the nonimmune IgG isotype control (Fig. 5A) , specific labeling for {alpha}vβ3 (Fig. 5B) and {alpha}vβ5 (Fig. 5C) integrins were detected on the surfaces of HSFs (P < 0.05), with the anti-{alpha}vβ5 antibody generating a stronger signal than the anti-{alpha}vβ3 antibody (Fig. 5D) . Binding of biotinylated rTGFBIp to HSFs in the presence of anti-{alpha}vβ3 antibody (Fig. 6A) and anti-{alpha}vβ5 (Fig. 6B) antibody was significantly inhibited at concentrations of 1 to 10 µg/mL (60%–84% and 42%–56%, respectively). The anti-{alpha}vβ5 antibody was less effective at inhibiting the binding of biotinylated rTGFBIp but still demonstrated a significant decrease in binding at concentrations ≥1 µg/mL (P < 0.05). After the binding assays, anti-{alpha}vβ3 and anti-{alpha}vβ5 integrin antibodies were confirmed, with the use of Western blot analysis, to bind to the surfaces of HSFs by detection of mouse IgG with anti-mouse IgG conjugated to alkaline phosphatase (data not shown).


Figure 5
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  		FIGURE 5. Integrin expression on the surface of HSFs. Flow cytometry on live HSFs incubated with 4 µg/mL IgG isotype control (A) or the monoclonal antibodies anti-{alpha}vβ3 (B) and anti-{alpha}vβ5 (C). Data are expressed as cell counts (y-axis) plotted as a function of fluorescence intensity (x-axis) and are representative of three independent experiments. (D) Histogram represents the mean intensities of anti-{alpha}vβ3 and anti-{alpha}vβ5 from flow cytometric analysis compared with the IgG isotype control. Data are expressed as mean ± SEM by the Student’s t-test for unmatched pairs for four individual experiments. *P < 0.05; **P < 0.01.

 

Figure 6
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  		FIGURE 6. TGFBIp binds to HSFs by interacting with {alpha}vβ3 and {alpha}vβ5 integrins. Representative Western blots of cell lysates collected from HSFs preincubated with the function-blocking monoclonal antibodies (0–10 µg/mL) against (A) {alpha}vβ3 and (B) {alpha}vβ5 for 1 hour at 4°C, before the addition of biotinylated rTGFBIp (10 µg/mL) for 5 hours at 4°C. Blots were probed with streptavidin conjugated to alkaline phosphatase (top), stripped and reprobed with {alpha}-tubulin antibody (bottom). Arrowhead: biotinylated rTGFBIp (~68 kDa). Histograms represent the relative band intensities quantified; each band was normalized to its corresponding {alpha}-tubulin. Data are expressed as mean ± SEM for three independent experiments in triplicate. *P < 0.05; **P < 0.01 using ANOVA with Bonferroni post-hoc correction.

 
Expression of TGFBIp and Integrins in HSFs
The distribution of TGFBIp, {alpha}vβ3, and {alpha}vβ5 was assessed on the surfaces of cultured HSFs with the use of immunocytochemistry (Fig. 7) . TGFBIp was predominantly expressed on the cell surface, between adjacent cells, with minimal intracellular expression and integrins {alpha}vβ3 and {alpha}vβ5 appeared to colocalize with TGFBIp on the cell surface (merged images). Acellular staining (Fig. 7) most likely represents areas in which cells had been artifactually detached during the procedure. Negative control sections were processed in parallel by incubation with secondary antibody only, or nonimmune mouse IgG, and showed no significant fluorescence signal.


Figure 7
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  		FIGURE 7. Colocalization of TGFBIp to {alpha}vβ3 and {alpha}vβ5 integrins in HSFs. Immunofluorescence of TGFBIp (red) on the surfaces of HSFs double labeled with anti-{alpha}vβ3 (green, middle), or with anti-{alpha}vβ5 (green, bottom). Right: merged images. Yellow: areas of colocalization. Nuclei are counterstained with DAPI (blue). No signal was detected in secondary antibody only or in nonimmune mouse IgG controls.

 

   Discussion
Top
 Abstract
 Methods
 Results
 Discussion
References
 
TGFBIp is primarily expressed in collagen-rich tissues in association with various extracellular matrix components and the cell surface, suggesting an organizational and structural role. TGFBIp is approximately 77 kDa in size and contains an NH2-terminal signal peptide sequence (residues 1–23) that is proteolytically processed during export to the ECM, rendering the protein a 68-kDa isoform.46 Additionally, this protein contains 11 cysteine residues mainly clustered in the NH2-terminal region (EMI domain), four highly conserved fasciclin-like (FAS) domains, and a COOH-terminal Arg-Gly-Asp (RGD) sequence.45 46 57 58 Because of the structural components of the protein, the presence of the FAS and RGD domains indicates that TGFBIp may play a functional role in cell adhesion.59 60 61 62 In marmoset and human sclera, TGFBIp expression has only recently been described.44 To elucidate the role of TGFBIp within the scleral extracellular matrix, studies in our laboratory have focused on the cell–matrix interactions using an in vitro system.

Results in the present study demonstrate that HSFs express TGFBI and that its protein product, TGFBIp, is secreted into the culture medium in abundant quantities by HSFs, in vitro (~833 ng/h). Relatively little TGFBIp remained attached to the cell surface or was contained intracellularly, as demonstrated by Western blot analyses of the 10x cell lysate (Fig. 1B) . Secreted TGFBIp was detected as a single 68-kDa band (Fig. 1B) , but a higher molecular weight band (~120 kDa) was present in cell lysates containing biotinylated rTGFBIp when probed with streptavidin-AP (Figs. 3 4 6) . Because this band was not present when blots were probed with anti-TGFBIp, we suspect this band represents nonspecific binding of streptavidin to a protein in the cell lysates.63 64

We previously demonstrated the inhibitory effect of TGFBIp on the attachment of HSFs in a solid-phase cell adhesion assay.44 The present study demonstrates that TGFBIp mediates decreased HSF attachment to collagen type I in a fluid-phase assay. Previous studies have shown TGFBIp supports cell adhesion in many cell types, including corneal fibroblasts,65 66 67 foreskin fibroblasts,62 bladder fibroblasts,68 U87 astrocytoma cells,69 skeletal muscle cells,70 proximal tubular epithelial cells,71 osteoblasts,53 keratinocytes,72 SMMC-7721 hepatoma cells,73 and peritoneal mesothelial cells.74 Conversely, it has been reported to inhibit cell adhesion in human neuroblastoma cells,75 A549 lung adenocarcinoma cells, HeLa cells, and WI-38 cells.46 In the present study, we determined that rTGFBIp inhibited the attachment of HSFs to collagen (–32%; P < 0.01), and this effect was restored after neutralizing rTGFBIp with equimolar amounts of anti-TGFBIp compared with BSA (+9%; P = 0.29; Fig. 2B ). Additionally, the short incubation period (45 minutes) allotted for cell attachment suggested that the anti-adhesive effect of rTGFBIp on HSFs was not a result of decreased cell proliferation. In agreement with previous reports, we observed that rTGFBIp did not inhibit attachment to collagen type I using HFFs (–4%; P = 0.50; Fig. 2C ) or HCFs (+37%; P = 0.24; Fig. 2D ), compared with BSA. However, a significant decrease in attachment to collagen type I was observed in HFFs treated with antibody-neutralized rTGFBIp compared with cells treated with BSA alone (–28%; P < 0.01). Because the attachment of HFFs to collagen type I was not affected by treatment with anti-TGFBIp alone, we speculate that the TGFBIp antibody/antigen complexes generated in vitro must have been anti-adhesive to HFFs in our attachment assays. Nevertheless, the finding that TGFBIp inhibits the attachment of HSFs, but not HFFs or HCFs, to collagen type I suggests multiple functional roles of TGFBIp among different cell and tissue types. It also suggests that the anti-adhesive effect of TGFBIp may be fairly specific for HSFs. In contrast to TFGBIp, FN enhanced the attachment of HSFs to collagen type I. We speculate that FN may attach to HSFs through the {alpha}vβ5 integrin receptor because FN has been demonstrated to bind to a variety of cell types by this receptor,76 77 78 and we have demonstrated this integrin on the HSF cell surface. Give that rTGFBIp was shown to bind to HSFs by both {alpha}vβ3 and {alpha}vβ5, it is likely that rTGFBIp may block the adhesion of HSFs to FN as well; however, these experiments were not conducted in the present study.

Several studies have reported that TGFBIp can bind to the surfaces of cells in connective tissue-rich matrices to modulate their adhesive properties through cell-specific integrins.47 53 62 68 69 73 79 80 In the present study, binding assays using biotinylated rTGFBIp (0–50 µg/mL) confirmed that TGFBIp binds directly to the surfaces of HSFs, and binding was saturable at concentrations ≥0.37 nM with an IC50 of 0.03 nM. Interestingly, this relatively high-affinity binding of TGFBIp to the HSF cell surface described here was similar to that described for the affinity of TGF-β1 latency-associated peptide binding to {alpha}vβ6 integrin receptors (18 pM).81 Integrins implicated in binding TGFBIp to the cell surface include, {alpha}1β1,82 {alpha}3β1,72 73 83 84 {alpha}Vβ3,53 74 {alpha}Vβ5,53 85 {alpha}7β1,70 and {alpha}6β4.69 The Arg-Gly-Asp (RGD) sequence present on the C-terminal region of TGFBIp is thought to act as a universal ligand recognition site for integrins; however, the attachment and spreading of cells to TGFBIp does not solely require the RGD sequence but can occur through fasciclin-like domains.82 In the present study, flow cytometry and immunocytochemistry using monoclonal antibodies to the integrins {alpha}vβ3 and {alpha}vβ5 were used to identify the expression of {alpha}vβ3 and {alpha}vβ5 on the HSF cell surface. Based on the mean fluorescence intensities, the relative expression level of {alpha}vβ5 appeared more elevated than that of {alpha}vβ3. Therefore, {alpha}vβ5 may function predominantly in mediating the binding of TGFBIp to HSFs. In addition to our findings, two previous reports in tree shrew, both in vitro and in vivo, have demonstrated mRNA expression of the integrin subunits, {alpha}1, {alpha}3, and β1 in scleral fibroblasts.86 87 Taken together, these results suggest that scleral fibroblasts express a variety of integrin subunits, a subset of which are translated and expressed as integrin receptors on the cell surface.

To identify whether {alpha}vβ3 or {alpha}vβ5 integrins play a role in TGFBIp binding to the surfaces of HSFs, additional binding assays were conducted after preincubation with specific antibodies to the {alpha}vβ3 and {alpha}vβ5 integrins (0–10 µg/mL). Binding of biotinylated rTGFBIp was significantly inhibited in a dose-dependent manner by the addition of anti-{alpha}vβ3 or anti-{alpha}vβ5. This disruption of interactions between TGFBIp and HSFs by function-blocking antibodies specific for {alpha}vβ3 and {alpha}vβ5 integrins suggests that {alpha}vβ3 and {alpha}vβ5 mediate some of the binding of TGFBIp to the HSF cell surface and, therefore, have the potential to regulate attachment.

The mechanism by which TGFBIp modulates cell attachment is not well understood. The results of this study suggest that {alpha}vβ3 and {alpha}vβ5 integrins are functional receptors for TGFBIp on the scleral cell membrane. The expression and activity of integrin downstream signaling molecules FAK and paxillin show a positive correlation with TGFBIp expression in human hepatoma cells, suggesting that TGFBIp may alter cell attachment through an integrin-mediated signaling cascade that may lead to cytoskeleton reorganization.73 Alternatively, the binding of TGFBIp to the HSF cell surface may sterically inhibit cell attachment to collagen type I, as has been demonstrated for hexabrachion (tenascin)88 and thrombospondin.89 90 91 In support of integrin-mediated signaling, FN was shown in the present study to enhance the attachment of HSFs to collagen type I. Because FN is well known to mediate its proadhesive property through the {alpha}vβ3 integrin receptor(s), it is possible that interaction differences between TGFBIp, FN, and the {alpha}vβ3 integrin receptor result in distinct downstream signaling pathways that lead to increased adhesion in one condition (FN) and decreased adhesion in another (TGFBIp). Moreover, differences in integrin subunit expression between different cell types may initiate divergent signaling cascades that result in TGFBIp becoming proadhesive for some cell types and anti-adhesive for others.

The highly regulated viscoelastic nature of the sclera has been speculated to occur as a result of slippage (creep) of the lamellae across each other at the cell-lamellae interface33 and is highly correlated with the rate of ocular elongation during myopia development and during decelerated ocular growth during recovery or compensation for plus lenses.33 34 Therefore, we speculate that changes in scleral ECM remodeling and cell–matrix interactions at the lamellae interface may modulate viscoelasticity in a variety of ocular growth states. The results presented in this article suggest that TGFBIp is one molecule that may regulate the attachment of HSFs to collagen type I at the fibroblast-lamellae interface, thereby regulating the amount of lamellar slippage and scleral viscoelasticity and the rate of scleral elongation. Interestingly, significant increases in TGFBI mRNA transcription levels were recently observed to occur in the scleras of tree shrew eyes undergoing minus-lens compensation.92 These results, together with the results of the present study, suggest that changes in scleral levels of TGFBIp may act to regulate ocular elongation through the modulation of cell–matrix interactions.

The molecular mechanisms that regulate scleral ECM remodeling, scleral distensibility, and axial length are poorly understood. Results of the present study suggest that TGFBIp may limit cell–matrix interactions between HSFs and collagen type I through integrin receptors. Additional functional in vivo studies are required to elucidate the roles of TGFBIp, {alpha}vβ3, and {alpha}vβ5 in the sclera and to determine how these proteins may be involved in scleral ECM remodeling during normal ocular growth and myopia development.


   Acknowledgements
 
The authors thank Brian de la Cruz and Rachel Folger for their technical assistance, and David M. Sherry and Brian P. Ceresa for their helpful discussions and suggestions pertaining to this manuscript.


   Footnotes
 
Supported by National Eye Institute Grant R01 EY09391 (JASR) and by the Macula Vision Research Foundation (JASR).

Submitted for publication January 26, 2009; revised March 7, 2009; accepted May 18, 2009.

Disclosure: L. Shelton, None; J.A. Summers Rada, None

The publication costs of this article were defrayed in part by page charge payment. This article must therefore be marked "advertisement" in accordance with 18 U.S.C. §1734 solely to indicate this fact.

Corresponding author: Jody A. Summers Rada, Department of Cell Biology, University of Oklahoma Health Sciences Center, 940 Stanton L. Young Boulevard, Oklahoma City, OK 73104; jody-summersrada{at}ouhsc.edu.


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