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(Investigative Ophthalmology and Visual Science. 2007;48:1061-1071.)
© 2007 by The Association for Research in Vision and Ophthalmology, Inc.
DOI:  10.1167/iovs.06-0772
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Inhibition of Human Corneal Epithelial Production of Fibrotic Mediator TGF-ß2 by Basement Membrane–Like Extracellular Matrix

Adriana J. LaGier,1 Sonia H. Yoo,1 Eduardo C. Alfonso,1 Sally Meiners,2 and M. Elizabeth Fini1

1From the Evelyn F. and William L. McKnight Vision Research Center, Bascom Palmer Eye Institute, University of Miami Miller School of Medicine, Miami, Florida; the 2Department of Pharmacology, Robert Wood Johnson Medical School, University of Medicine and Dentistry of New Jersey, Piscataway, New Jersey.


   Abstract
Top
 Abstract
Materials and Methods
 Results
 Discussion
 References
 
PURPOSE. Transforming growth factor (TGF)-ß2 is a major epithelial mediator of fibrotic marker expression during corneal repair in mice. Production of TGF-ß2 protein by cultured rabbit corneal epithelial cells is reduced by plating on a basement membrane–like extracellular matrix extract (Matrigel; BD Biosciences, Bedford, MA). The goal of the present study was to understand further the nature of Matrigel regulation.

METHODS. TGF-ß2 protein, mRNA, and gene transcriptional promotion were characterized in cultured human corneal epithelial cells.

RESULTS. TGF-ß2 production was inhibited by Matrigel at the level of mRNA accumulation and activity of the gene transcriptional promoter. This effect of Matrigel was not explained by (1) growth factor contaminants, as growth-factor reduced Matrigel also inhibited TGF-ß2; (2) independent matrix components, as the pure forms of the major ECM components laminin and collagen IV did not reproduce the effect; or (3) inhibition of a constitutive TGF-ß2 autocrine feedback loop, as addition of exogenous TGF-ß2 increased p-Smad3 and restored TGF-ß2 mRNA levels. In addition, Matrigel’s ability to reduce TGF-ß2 was not explained by its geometry, as TGF-ß2 production was not inhibited by plating cells on a synthetic nanofiber matrix with a three-dimensional topography similar to Matrigel. Matrigel caused a reduction of ezrin, a member of the ezrin-radixin-moesin (ERM) family, which plays a role in establishing polarity of epithelial cells in tissues through the Rho signaling pathway.

CONCLUSIONS. These findings indicate that Matrigel inhibits TGF-ß2 gene expression and point to a mechanism dependent on Matrigel composition and structure. The capacity of Matrigel to reduce ezrin is consistent with this idea and directs the focus of future studies toward the ERM/Rho pathway.

Penetrating injuries in adult mammals are typically repaired via a fibrotic response, initiated by a diverse array of cytokines released into the wound environment that stimulate cells to divide, reorganize actin into stress fibers, express new repair-associated proteins, and deposit extracellular matrix.1 2 3 4 The fibrotic tissue repair response results in a rapid filling of space, which can be organ saving and life saving, but does not regenerate function. However, under some circumstances, the repair response to injury can be quite regenerative (e.g., in the first embryonic trimester).5 Studies comparing regenerative and fibrotic repair have implicated transforming growth factor (TGF)-ß as a key cytokine involved in giving repair tissue its fibrotic character.6 7 8 Pharmacologic agents that target TGF-ß activity have been effective in giving repair a more regenerative character with less scarring.5 7

Cellular changes of repair are controlled in skin by proteins that are released from platelets, including platelet-derived growth factor (PDGF) and TGF-ß.9 Like skin, the cornea is composed of a collagenous stroma surfaced by epithelial cells, but unlike skin, it contains no blood vessels, and thus there are no platelets to serve as the source of repair cytokines. Yet corneal injuries due to trauma or surgical procedures that penetrate the epithelial basement membrane and Bowman’s layer typically stimulate a fibrotic repair response that results in deposition of a "hazy" repair tissue that interferes with corneal clarity.8 The clinical impression has been that the epithelium may be a major source of cytokines controlling fibrosis in the cornea.10 Recently, our research group determined that the epithelial cells of the cornea substitute for platelets in controlling the fibrotic phenotype by producing TGF-ß—in the mouse, specifically, the isoform TGF-ß2. We have further shown that the release of TGF-ß2 from the mouse corneal epithelium and activation of fibrotic gene expression in corneal stromal repair cells correlates in vivo with the absence of basement membrane.11 12 Therefore, epithelial TGF-ß2 appears to be a key modulator of fibrotic repair in the cornea when epithelial-stromal interactions are initiated after penetrating injuries disrupt the basement membrane.

Epithelial cells, including those from cornea, produce many regulatory cytokines (reviewed in Ref. 13 ). The net effect on the underlying mesenchymal tissue is due to the sum of activities released. In a study to understand how corneal epithelial cells control collagenase synthesis by corneal stromal cells, we identified the major stimulator as IL-1{alpha} and the major inhibitor as TGF-ß2.14 15 The mechanism regulating the release of each cytokine was quite different. IL-1{alpha} release was inversely related to cell density, released at much higher rates in cells with limited contact. In contrast, release of TGF-ß2 was not affected by cell density.15 However, the findings just described that have implicated basement membrane in control of fibrosis suggest that this may be the determinant of TGF-ß2 release. We investigated the role of basement membrane in a rabbit corneal epithelial cell culture model12 and confirmed our hypothesis, showing that epithelial cells produce much less TGF-ß2 protein when plated on Matrigel, a complex basement membrane–like extracellular matrix extract.

Pharmacologic targeting of TGF-ß2 production by corneal epithelial cells could be a novel means for improving the regenerative quality of repair.16 17 The goal of the present study was to explore this initial finding concerning Matrigel regulation of TGF-ß2, so as to acquire information necessary for development of a pharmacologic strategy. We developed and applied a human corneal cell culture model for these new investigations, to increase the clinical relevance.


   Materials and Methods
Top
 Abstract
 Materials and Methods
Results
 Discussion
 References
 
Corneal Tissue and Cell Lines
Central corneal tissue was obtained from the National Disease Research Interchange (Philadelphia, PA). Human donor corneoscleral rims preserved in Chen’s medium were provided by the Florida Lions Eye Bank located at the Bascom Palmer Eye Institute in accordance with the guidelines in the Declaration of Helsinki for research involving human tissue. Mink lung epithelial (Mv1Lu) cells were obtained from American Type Culture Collection (Manassas, VA) and cultured as recommended.

Human Corneal Epithelial Cell Culture
Human corneal epithelial cells (HCECs) were derived from human donor corneoscleral rims by a previously described method.18 Briefly, sclera and iris remnants were trimmed from each corneoscleral rim, and each rim was dissected into eight equal segments. Each segment was then placed in 1 well of a 24-well culture plate (Nunclon; Nalge Nunc International, Naperville, IL). The explant was treated with 2.5% wt/vol Dispase for 15 minutes at 37°C, washed, and cultured in keratinocyte-serum-free medium (SFM; Invitrogen, Carlsbad, CA), a low calcium, serum-free medium. The manufacturer provides epidermal growth factor (EGF) and fibroblast growth factor (FGF)-2 to be added as supplements to stimulate cell growth, but we did not use these particular supplements, instead substituting 10% fetal bovine serum (FBS). The medium was also supplemented with 50 U/mL penicillin, 50 µg/mL streptomycin, and 0.5 µg/mL amphotericin B at 37°C under 95% humidity and 5% CO2. After 3 weeks, epithelial cells from three rims, or a total of 24 segments (1.5 x 106 ± 0.3 x 106 cells), were ready for experiments.

For the experiments, HCECs were trypsinized, pooled, and seeded onto plastic tissue culture dishes (Nunclon; Nalge Nunc International) at a density of 104 cells per well of a 96-well plate or 105 cells per well of a 24-well plate. Cells plated at this density were approximately 50% confluent. The same medium used for explant culture was used in the experiments, but without addition of serum or any other mitogens, to minimize cell proliferation and to avoid the confounding factor of extracellular matrix (ECM) proteins present in serum.19 More than 95% of the plated cells were viable, as assessed by trypan blue. In addition, essentially all the cells stained positive for cytokeratin-3 (clone AE5; Chemicon, Temecula, CA), confirming that they were epithelial cells (see Figs. 1 3 ).


Figure 1
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  		FIGURE 1. Prominence of the TGF-ß2 isoform in the human corneal epithelium and cultured HCECs. TGF-ß1 or -ß2 isoforms were localized on paraffin-embedded sections from human central cornea (A) or cultured HCECs (B, C) by indirect immunofluorescent staining with primary antibodies to TGF-ß1 or -ß2, including a control without primary antibody. Staining with cytokeratin 3 antibody was used as a corneal epithelial marker. Green: positive staining; red: nuclei counterstained with propidium iodide. Brackets: corneal epithelial layer; arrow: location of the epithelial basement membrane. HCECs were plated at a density of 104 per well on a 96-well plate and cultured overnight in serum-free medium before immunostaining. The sections were photographed with a 10x or 40x microscope objective; the cells were photographed with a 40x microscope objective.

 

Figure 3
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  		FIGURE 3. Matrigel reduces TGF-ß2 protein production in a time-dependent manner in HCECs. HCECs were plated in serum-free medium for 1, 3, 5, or 7 days at a density of 104 or 105 per well on 96- or 24-well plates, respectively, coated with laminin (LM) or GFR-Matrigel (rM). The cells remained subconfluent throughout the time course because they were cultured without serum, minimizing cell proliferation. Cell counts made from representative fields such as shown in (B) indicated that the number of cells neither increased nor decreased during the 7-day period. (A) Immunoblots of cytoplasmic lysates probed with TGF-ß2 antibody, then stripped and reprobed with ß-actin antibody (top). Graph of immunoblot data (bottom). Relative TGF-ß2 protein was determined as a ratio of the TGF-ß2 to the ß-actin band densities and is compiled from two independent experiments (average ± high/low). *P < 0.05, GFR-Matrigel versus laminin. (B) Localization of TGF-ß2 protein in the HCECs at day 1 or 7 after plating by indirect immunofluorescent staining. A control without primary antibody for nonspecific staining was included (No Primary). Staining with cytokeratin 3 antibody was used as a corneal epithelial marker. Green: positive staining; red: nuclei counterstained with propidium iodide. (C) Immunoblots of conditioned media probed with TGF-ß2 antibody (top). Graph of immunoblot data (bottom). TGF-ß2 protein values were determined from the TGF-ß2 band densities per 5 µg total protein and are compiled from two independent experiments (average ± high/low). Recombinant human TGF-ß2 (10 ng; T) was run as a positive control. TGF-ß2 bands from lysates are 25 kDa and from conditioned media are 95 kDa, and ß-actin bands are 42 kDa based on molecular size markers (not shown). *P < 0.05, GFR-Matrigel versus laminin.

 
For experiments examining ECM’s effects on TGF-ß2 expression, the wells were left untreated or precoated with 10 µg/cm2 of specific ECM substrates: BD Matrigel matrix (BD Biosciences, Bedford, MA), or growth factor–reduced (GFR) BD Matrigel matrix (GFR-Matrigel), laminin, fibronectin, or collagen type IV, all obtained from BD Biosciences (Bedford, MA). Matrigel is a solubilized basement membrane preparation extracted from the Engelbreth-Holm-Swarm mouse sarcoma, a tumor rich in ECM proteins. Its major component is laminin, followed by collagen IV, heparan sulfate proteoglycan (primarily perlecan), entactin, and nidogen. It also contains some proteinases, TGF-ßs, and other growth factors naturally present in the tumor. At room temperature, Matrigel polymerizes to produce a biologically active matrix material resembling the mammalian cellular basement membrane. GFR-Matrigel is useful as an alternative to Matrigel when a more highly defined basement membrane preparation is desired. The product is a 20% ammonium sulfate-extracted version of Matrigel.20 Most of the major ECM components of Matrigel are conserved by the process except for heparan sulfate proteoglycan, which is reduced by 40% to 50%. Extraction selectively targets low-molecular-weight proteins, thus effectively removing growth factors except for TGF-ßs which may be bound to collagen IV and/or sequestered in a latent form that partitions with the major components in the purification procedure. In some of our experiments, GFR-Matrigel, which has ~1.7 ng/mL residual TGF-ß2, was pretreated with antibody to neutralize the TGF-ß2 (R&D Systems, Minneapolis, MN), 0.3 µg/mL per 1 ng/mL TGF-ß in GFR-Matrigel.

To ensure that cell attachment occurred with equal efficiency on the different ECM coatings, we stained the cells with a fluorescent staining reagent (Cyquant; Invitrogen) and counted them. The results indicated that cell adherence occurred equally on plastic and on the different ECM coatings used in our experiments (data not shown).

For experiments requiring plating of cells on coverslips, 12-well dishes were used. These experiments used Aclar (polychlorotrifluoroethylene [PCTFE], Honeywelll Specialty Materials, Morristown, NJ) coverslips electrospun with polyamide nanofibers, with or without amines (Ultra-Web; Donaldson Co., Inc., Minneapolis, MN), and coated by SurModics (Eden Prarie, MN).21 Aclar coverslips were used instead of glass because of the need to ship the coverslips from New Jersey to Miami with their preservation in an intact state. No major differences in terms of cell morphology or function have been noted between cells cultured on Aclar and those cultured on glass (S. Meiners, unpublished data, 2005).

Immunostaining
Tissue was formalin fixed, paraffin processed, sectioned, cleared, and rehydrated. The cultured cells were methanol fixed. The cells were immunostained with (1) mouse anti-human cytokeratin 3 (clone AE5; Chemicon); (2) rabbit antibodies against human TGF-ß1, TGF-ß2 (Santa Cruz Biotechnology, Santa Cruz, CA), Smad3 (Upstate, Lake Placid, NY), or ERM (Cell Signaling, Beverly, MA); or (3) no primary antibody (all diluted 1:50), and detected with Alexa-Fluor 488 conjugated anti-mouse or anti-rabbit antibody (Invitrogen). Nuclei were counterstained with propidium iodide (Roche, Indianapolis, IN).

To quantify the percentage of positive cells, we viewed four fields of HCECs (≥200 cells per field) by fluorescence microscope with the 10x objective. Positively stained cells were counted in each field, and total propidium iodide–stained nuclei were counted as a measure of the total number of cells. Counts obtained from each field were then averaged, and the ratio of positive cells to total cells was calculated. The statistical significance of differences between experimental groups was determined by Student’s t-test (Origin software; OriginLab, Northhampton, MA).

Quantitative Reverse Transcription–Polymerase Chain Reaction
Total RNA was extracted from the cells with a total aurum kit, as per the manufacturer’s instructions (Bio-Rad, Hercules, CA). Total RNA was quantified spectrophotometrically at 260 nm, and 10 ng/µL RNA was reverse transcribed (iScript cDNA Synthesis Kit; Bio-Rad). One-tenth of the cDNA was subjected to qRT-PCR (iQ SYBR Supermix; Bio-Rad) and primers developed for 18S rRNA or GAPDH and TGF-ß2 (TGFß2-F [forward], 5'-GACCCCACATCTCCTGCTAA-3'; TGFß2-R [reverse], 5'-AGGCAGCAATTATCCTGCAC-3') (Invitrogen) on a thermocycler (iCycler; Bio-Rad). We developed the TGF-ß2 primers, mouse TGF-ß2 (BC011170, gi:15029891) 957-1082, to cross exon 5, which is shared by rabbit (AY429466, gi:37993795), mouse, and human (AY438979, gi:37953286) and contains the putative cut site between latency-associated protein (LAP) and mature TGF-ß2. Melting curves indicated that the primer sets produced one product. TGF-ß2 levels expressed as threshold cycles were normalized to an internal control: 18S or GAPDH. Relative TGF-ß2 mRNA was calculated as a ratio of TGF-ß2 to the 18S threshold cycles using the thermal cycler system software (iCycler iQ Optical System Software, ver. 3.0a; Bio-Rad).

TGF-ß2 Reporter Construct and Transcriptional Activity Assay
TGF-ß2 promoter DNA was generated by PCR from a 1q41 BAC, RP11-224O19 (Children’s Hospital Oakland Research Institute, Oakland, CA). The primers (TGF-ß2 promoter-F, 5'-GAAAGATGCTCACTGGCTTG-3'; TGF-ß2 promoter-R, 5'-TTGTTGTTTTTGATGCGAAACT-3') (Invitrogen) were used to create a 3,230-bp product between 50,731 and 53,961 on RP11-224O19 that corresponds to the sequence for the TGF-ß2 promoter, –40 to –3270 upstream of the start of exon 1 (M87843, gi:339565) and includes the transcriptional start site at 52,705 and the TATA box at 52,673.22 This TGF-ß2 promoter DNA was TA cloned (GeneBlazer technology; Invitrogen) and inserted upstream of a ß-lactamase enzyme gene (pcDNA6.2/cGeneBlazer-GW/D-TOPO; Invitrogen). The reporter construct was confirmed by primer walking sequencing (GeneWiz, New Brunswick, NJ).

Using a ubiquitin-C-bla(M) (UBC-bla[M]) vector (Invitrogen), we determined that the bla(M) reporter construct approach would work in HCECs and that transfection occurred in ~15% to 20% of the HCECs. The DNA coding for the human TGF-ß2 promoter was linked to the ß-lactamase (bla[M]) reporter gene to create the TGFb2-bla(M) construct. The capacity of our TGF-ß2 promoter construct to drive bla(M) expression was confirmed in Mv1Lu cells, which have been shown to promote TGF-ß on exposure to TGF-ß (see Fig. 4B ).23


Figure 4
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  		FIGURE 4. Matrigel inhibits TGF-ß2 gene transcriptional promoter activity in HCECs. HCECs were plated in serum-free medium at a density of 104 or 105 per well on 96- or 24-well plates, respectively, that were left uncoated (P) or coated with laminin (LM) or GFR-Matrigel (rM). After overnight culture, the cells were transfected with the indicated (bla[M]) reporter vectors and analyzed 48 hours later for reporter expression. (A) Demonstrating the range of the reporter assay is a representative micrograph of HCECs plated on plastic depicting UBC-bla(M) promoter activity (blue) versus empty bla(M) vector controls (green). (B) To validate the promoter assay, Mv1Lu cells plated on plastic were treated without (–, {square}) or with (+, Figure 4) 10 ng/mL of recombinant human TGF-ß2 for 1 day after transfection with bla(M) vectors. Relative bla(M) activity is calculated as a ratio of the TGFb2-bla(M) to the empty-bla(M) fluorescence units and represents quadruplicate determinations (average ± SD). (C) HCECs were transfected with either empty-(bla[M]) or TGFb2-(bla[M]) vector and loading with a green fluorescent dye, CCF-AM, 48 hours later. A representative micrograph from one of three independent experiments depicts that HCECs fluoresce blue when TGF-ß2 gene transcriptional promoter activity is positive and remain green when it is negative. As shown in the histogram, fluorescence was quantified and calculated as relative bla(M) activity. (D) In additional experiments addressing the question of transfection efficiencies, HCECs were cotransfected with reporter constructs, empty-bla(M) or TGFß2-bla(M), and a dsRed vector at a 5:1 ratio. Bla(M) activity (%) indicates the percentage of successfully transfected HCECs, red cells, which had positive TGF-ß2 gene transcriptional promoter activity, blue cells. Bla(M) activity (%) is calculated for triplicate fields of view (average ± SD). *P < 0.05, GFR-Matrigel versus laminin.

 
The TGF-ß2 reporter construct (TGFb2-bla(M)) or empty vector (empty-bla[M]) was introduced into HCECs in serum-free conditions (Transfectin; Bio-Rad), as per the manufacturer’s instructions. Two days after transfection, cells were loaded with a green fluorescent substrate, CCF2. Green fluorescence and blue fluorescence, a measure of TGFb2-bla(M) gene transcriptional activity, was visualized by an inverted scope equipped with long-pass filters 460/520 nm (Filter 41031; Chroma, Technology Corp., Rockingham, VT) and quantified by a fluorescence plate reader (BioTek, Winooski, VT). The ratio of blue to green fluorescence signal was obtained by dividing the 460-nm emission (blue) reading by the 530-nm emission (green) reading after the background fluorescence obtained at each wavelength was subtracted.

In additional experiments, we ensured that transfection occurred with equal efficiency on the different ECM coatings. HCECs were cotransfected with our reporter constructs—empty-bla(M) and TGFb2-bla(M)—and a dsRed vector at a 5:1 ratio. We counted the percentage of successfully transfected HCECs (red cells) that were positive for TGF-ß2 gene transcriptional activity (blue cells).

Immunoblot Analysis
Cell lysates were prepared in lysis buffer (50 mM Tris, 1% Triton X-100, 0.1% SDS, 0.5% deoxycholate, 150 mM NaCl, 10 µg/mL aprotinin [Roche], leupeptin [Roche], and 5 mM sodium orthovanadate [Sigma-Aldrich, St. Louis, MO]). Lysates and conditioned media were cleared by centrifugation, and protein concentrations were determined with a protein assay (Bio-Rad), according to the manufacturer’s instructions. Samples with 5 to 10 µg total protein were subjected to SDS-polyacrylamide gel electrophoresis on 10% to 15% Tris-glycine gels (Bio-Rad) and electroblotted onto polyvinylidene fluoride (PVDF) membranes (Immobilon; Millipore, Billerica, MA). A molecular weight standard (Cruz Marker; Santa Cruz Biotechnology) that consists of six bands (132, 90, 55, 43, 34, and 23 kDa) was used as an internal size standard. The membranes were blocked with 5% dry milk or normal goat serum (NGS) in Tris-buffered saline (TBS)/Tween20 and probed with (1) 1:500 of anti-TGF-ß2 antibody (Santa Cruz Biotechnology) in 1% dry milk, (2) 1:500 of anti-phospho-Smad3 (pS423/425) antibody (Biosource, Camarillo, CA) in 1% NGS, or (3) 1:1000 of ezrin-radixin-moesin (ERM) antibody (Cell Signaling Technology, Beverly, MA) in 1% NGS, followed by incubation with horseradish peroxidase (HRP)–linked anti-rabbit antibody (Jackson ImmunoResearch, West Grove, PA). HRP was visualized by enhanced chemiluminescence (Sigma-Aldrich). The blots were stripped (Pierce Biotechnology, Rockford, IL) and reprobed with, respectively, (1) 1:2000 of anti-ß-actin (Sigma-Aldrich) in 1% dry milk or NGS, or (2) 1:500 of anti-Smad 2/3 (BD Biosciences), followed by incubation with HRP-linked anti-mouse or rabbit antibody (Jackson ImmunoResearch) and visualized as above. The TGF-ß2, phospho-Smad3 and ERM protein levels were normalized to internal ß-actin or Smad2/3. Protein levels were quantified as total adjusted volume of bands corrected for background (Quantity One software, ver. 4.4.1; Bio-Rad).

Data Presentation and Analysis
All data presented in graphs represent one of two or three experiments with similar results. Data are the mean ± SD from at least triplicate samples from a representative experiment. Statistical analysis, ANOVA or Student’s t-test, was performed (Origin Software; Origin Laboratory).


   Results
Top
 Abstract
 Materials and Methods
 Results
Discussion
 References
 
Prominence of the TGF-ß2 Isoform in the Human Corneal Epithelium and Cultured HCECs
Past reports have localized TGF-ß isoforms in human corneas and cultured HCECs24 25 26 27 28 29 30 ; however, these studies did not directly compare the relative levels of each isoform in the different corneal tissues. To ensure that our previous findings in mouse/rabbit,12 on the prominence of the TGF-ß2 isoform in the epithelium could be extended to the human species, we repeated our experiments in the new model (Fig. 1) . Immunoreactive protein for both isoforms was found in epithelium and stroma. However, as we previously observed in the mouse,12 TGF-ß2 was strikingly localized to the epithelium, whereas TGF-ß1 was primarily concentrated in the stroma (Fig. 1A) . In addition, HCECs grown out of corneoscleral rims and plated on plastic without serum were strongly TGF-ß2 positive, showing only a minimal TGF-ß1 immunoreaction, similar to that seen in the whole epithelium (Fig. 1B) . The HCECs were also cytokeratin 3/12 positive, indicating that they are mature central corneal epithelial cells31 (Fig. 1C) . These experiments indicated that the human pattern of TGF-ß1/TGF-ß2 localization in human corneas and cultured HCECs is the same as we found in mouse and rabbit,12 with TGF-ß2 being the prominent epithelial isoform.

Effect of GFR-Matrigel on TGF-ß2 Production at the Level of Steady State mRNA and Transcriptional Promoter Activity
We previously determined that plating of corneal epithelial cells on Matrigel leads to a significant reduction in the amount of TGF-ß2 protein produced.12 Matrigel is a complex mixture of ECM proteins, the major component being laminin, followed by collagen IV (approximately 60% and 30% by weight respectively, according to the manufacturer). Matrigel also contains heparan sulfate proteoglycans, as well as TGF-ßs and other growth factors that occur naturally in the tumor from which it is extracted. Using a fractionation approach, we sought to determine whether a specific component of Matrigel could mediate Matrigel’s effects on TGF-ß2 production by corneal epithelial cells. At the same time, we took one step back in the sequence of events in TGF-ß2 gene expression to determine whether Matrigel also reduces the steady state levels of TGF-ß2 mRNA. We started by comparing cells plated on plastic or Matrigel to those plated on GFR-Matrigel, an ammonium sulfate-extracted product with reduced levels of growth factors and about half the amount of heparin sulfate proteoglycan. In addition, we compared Matrigel to purified laminin and collagen IV. For comparison, we also compared Matrigel to fibronectin, a major component of the "provisional matrix" on which corneal epithelial cells migrate in corneal wound (reviewed in Ref. 32 ). HCECs were plated on these substrates, and the intracellular levels of TGF-ß2 mRNA were assayed 24 hours later by qRT-PCR.

Representative results of this set of experiments are shown in Figure 2 . Plating on Matrigel reduced the steady state level of intracellular TGF-ß2 mRNA by ~35% (rM 64.5% ± 2.6% of plastic control) compared with plastic (Fig. 2) . A similar result was obtained when HCECs were plated on GFR-Matrigel, with no significant difference compared with cells on Matrigel (Fig. 2) . In contrast, plating on purified laminin (Fig. 2) , collagen IV (Fig. 2B) , or fibronectin (Fig. 2B) had no significant effect on the TGF-ß2 mRNA level compared with plastic.


Figure 2
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  		FIGURE 2. Reduction in TGF-ß2 mRNA levels in HCECs plated on Matrigel, GFR-Matrigel, or TGF-ß2 inactivated GFR-Matrigel, but not purified laminin, collagen IV, or fibronectin. HCECs were plated in serum-free medium at a density of 105 cells per well in 24-well plates. The HCECs were plated on uncoated plastic (P) or on plastic coated with the following ECMs: Matrigel (M), GFR-Matrigel (rM), GFR-Matrigel pretreated with neutralizing antibody to TGF-ß2 (rM*), laminin (LM), collagen type IV (col-IV), or fibronectin (FN). Total RNA was harvested after 24 hours and subjected to qRT-PCR. The relative TGF-ß2 mRNA was calculated as a ratio of TGF-ß2 to the 18S threshold cycles and represents triplicates (average ± SD) from one of three experiments. Results of two representative experiments are shown. *P < 0.05 for (A) M and rM versus plastic; (B) rM and rM* versus plastic.

 
Although the levels of most growth factors is reduced in GFR-Matrigel, TGF-ß levels remain high enough (averaging 1.7 ng/mL) that there is the potential for it to affect TGF-ß2 production if the growth factor is in an active form. To rule out involvement of TGF-ß endogenous to Matrigel in mediating Matrigel’s inhibitory effect, we treated GFR-Matrigel-coated plates with an anti-TGF-ß2 neutralizing antibody before plating HCECs. Despite this neutralization, the level of TGF-ß2 mRNA was the same when HCECs were plated on GFR-Matrigel (rM) or neutralized reduced-Matrigel (rM*; Fig. 2B ).

The intracellular level of a specific protein is determined by its rate of synthesis and degradation. If TGF-ß2 production is controlled by Matrigel at the level of intracellular TGF-ß2 mRNA, then reduction in the level of intracellular TGF-ß2 protein should follow the reduction in intracellular mRNA. To examine this point, we observed the time course of the Matrigel-mediated reduction of intracellular TGF-ß2 protein levels by using the immunoblot assay. Representative results are shown in Figure 3 . As previously observed in the rabbit model, Matrigel reduced the intracellular level of TGF-ß2 protein in HCECs—in this case in comparison to laminin. However, in contrast to our finding that the reduction in the intracellular mRNA level occurred within 24 hours, the reduction in protein level was not observed until day 5 after plating and was maintained at day 7 (Fig. 3A) . The reduction in the level of intracellular TGF-ß2 at day 7 could also be observed by immunostaining (Fig. 3B) . Immunoblots of culture medium conditioned by the same cells analyzed for intracellular protein also revealed a Matrigel-mediated, time-dependent reduction in the level of TGF-ß2 accumulated in the culture medium (Fig. 3C) . Cell counts made from representative fields such as shown in Figure 3C indicated that the number of cells neither increased nor decreased during the 7-day time period. However, the cell morphology did change, a phenomenon previously described as epithelial cells plated on Matrigel polarize.33 These results are consistent with the idea that Matrigel acts to regulate the level of steady state TGF-ß2 mRNA.

The intracellular steady state level of a specific mRNA is determined by the rate of its transcription, processing, and degradation. The rate of transcription is determined primarily by the rate of transcriptional promoter activity. We investigated whether Matrigel inhibits transcriptional promoter activity of the TGF-ß2 gene. To do this, we used a transcriptional promotion assay that makes use of a bla(M) reporter gene construct. Representative results are shown in Figure 4 . To perform the assay, cells are transfected with a reporter gene construct and then loaded with the green fluorescent dye CCF-AM. If the transcriptional promoter is active, ß-lactamase is expressed, and the dye is enzymatically cleaved to produce a blue fluorescent product, as shown (Fig. 4A) . We created a TGF-ß2 reporter construct that was validated by showing its responsiveness to TGF-ß2 when transfected into Mv1Lu cells (Fig. 4B) . This construct was transfected into HCECs plated on either plastic, Matrigel, or purified laminin. As judged subjectively by the level of blue versus green fluorescence, TGF-ß2 promoter activity was high in cells plated on plastic or laminin, but low in cells plated on Matrigel. This difference was quantified using a fluorescence plate reader and was statistically significant (Fig. 4C) .

We ran additional experiments to demonstrate that transfection efficiency did not impact our findings. HCECs were cotransfected with reporter constructs and a dsRed vector. The percentage of successfully transfected HCECs, red cells, which had positive TGF-ß2 gene transcriptional promoter activity, blue cells was quantified (Fig. 4D) . Matrigel reduced the number of successfully transfected cells that had active transcriptional promotion of the TGF-ß2 gene.

These results indicate that (1) Matrigel reduces both the steady state levels of TGF-ß2 mRNA and the activity of the TGF-ß2 transcriptional promoter in corneal epithelial cells, as previously observed for TGF-ß2 protein production; (2) the growth factor contaminants and heparin sulfate proteoglycans present in Matrigel can be reduced without altering this effect; (3) neither laminin nor collagen IV—the two major components of Matrigel—is individually sufficient to mediate this effect.

Failure to Implicate TGF-ß2 Autocrine Loop Inhibition as the Matrigel Mechanism
TGF-ßs can regulate activity of the TGF-ß genes in cells that produce them via an autocrine feedback loop.25 We have previously shown that much of the TGF-ß2 produced by rabbit corneal epithelial cells in culture is in the biologically active form14 15 suggesting that it could serve as an active autocrine cytokine. Therefore, it could be hypothesized that HCECs maintain a positive TGF-ß2 autocrine feedback loop and that Matrigel acts to reduce TGF-ß2 levels by interfering with this loop. In fact, the Matrigel component collagen IV has been reported to bind and sequester TGF-ß2,34 providing a possible mechanism. We investigated this hypothesis in a set of experiments, of which representative results are shown in Figure 5 .


Figure 5
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  		FIGURE 5. Failure to implicate TGF-ß2 autocrine loop inhibition in mediating Matrigel reduction of TGF-ß2 expression in HCECs. HCECs were plated overnight in serum-free medium at a density of 105 per well on 24-well plastic dishes coated with GFR-Matrigel (rM) or laminin (LM). (A) Cells were subjected to indirect immunostaining for SMAD3. The smad3 antibody was omitted from the No Primary experiments as a control. Green: positive staining; red: nuclei counterstained with propidium iodide. (B) Immunoblotting of cytoplasmic lysates for phosphorylated (active) SMAD3 (p-SMAD3) and SMAD2/3 protein from HCECs plated overnight on laminin (LM) or GFR-Matrigel (rM) without (–) or with (+) a 15- or 30-minute treatment with recombinant human TGF-ß2 (10 ng/mL) before harvesting lysates. Top: a lysate from Mv1Lu treated with TGF-ß2 (Mv1Lu+) was run as a positive control. Bottom: relative protein is a ratio of the p-SMAD3 to the SMAD2/3 band densities and is compiled from two independent experiments (average ± high/low). p-SMAD3 bands are 50 kDa and SMAD2/3 bands are 58 kDa, based on molecular weight markers (not shown). (C, D) Culture medium was supplemented without (–) or with (+) 10 ng/mL recombinant human TGF-ß2. (C) Total RNA was harvested after 24 hours and subjected to qRT-PCR. The "relative TGFb2 mRNA" is calculated as a ratio of the TGF-ß2 to the loading control threshold cycles and represents triplicates (average ± SD) from one of two experiments. (D) Cells were transfected with either empty-(bla[M]) or TGFb2-(bla[M]) vector. Relative bla(M) activity is calculated as a ratio of the TGFb2-bla(M) to the empty-bla(M) fluorescence units and represents quadruplicate determinations (average ± SD) from one of two experiments. *P < 0.05, GFR-Matrigel versus laminin.

 
Signal transduction molecules of the Smad family mediate TGF-ß signaling and Smad3 participates in activation of the TGF-ß2 transcriptional promoter. HCECs plated on either GFR-Matrigel or laminin contained immunoreactive Smad3 protein (Fig. 5A) . The level of active phosphorylated Smad3 (p-Smad3) in HCECs plated on GFR-Matrigel was the same as in HCECs plated on laminin, as determined by immunoblotting (Fig. 5B) . However, treatment of HCECs with TGF-ß2 (10 ng/mL) for 15 or 30 minutes caused an increase in p-Smad3 in HCECs plated on either GFR-Matrigel or laminin.

When HCECs plated on GFR-Matrigel were treated with recombinant human TGF-ß2, the mRNA level for TGF-ß2 increased to the level observed in HCECs cultured on purified laminin (Fig. 5C) . Treatment with exogenous TGF-ß2 did not further increase TGF-ß2 mRNA levels in HCECs plated on laminin, suggesting that the cells were already making the highest possible amount. Of note, addition of exogenous TGF-ß2 did not rescue the reduction inTGF-ß2 promoter activity that occurred when cells were plated on GFR-Matrigel (Fig. 5D) .

These data indicate that Matrigel does not inhibit the ability of exogenous TGF-ß2 to initiate a signal cascade that leads to increased levels of steady state TGF-ß2 mRNA. Moreover, unlike Matrigel, exogenous TGF-ß2 does not affect the activity of the TGF-ß2 promoter, suggesting different control mechanisms. These results fail to support the hypothesis that Matrigel reduces TGF-ß2 production by reducing activity of an autocrine TGF-ß2 feedback loop.

Effect of Basement Membrane–like Topography on TGF-ß2 Production
Failing to find evidence to support an indirect mechanism of Matrigel-mediated reduction of TGF-ß2 production involving inhibition of a TGF-ß2 autocrine loop and also failing to identify a direct mechanism involving specific molecular components of Matrigel, we considered more complex possibilities. Recent work has provided evidence that the highly porous nanotopography that results from the three-dimensional (3-D) associations between ECM molecules that compose basement membranes activates signal transduction cascades in cultured cells.35 Therefore, we hypothesized that the 3-D architecture of Matrigel, as polymerized on coated tissue culture plastic, is responsible for the inhibition of TGF-ß2 production by HCECs plated on its surface.

One of our laboratories (Meiners) has developed 3-D synthetic nanofibrillar surfaces that mimic the porosity, geometry, and complexity of the extracellular matrix.36 Plating of cells on this surface activates Rac, a member of the Rho family of small GTPases.37 This signaling pathway is vital to cell morphology and cell–cell interactions and has been implicated in TGF-ß signaling.38 39 HCECs were plated on these surfaces, created on Aclar coverslips electrospun without (std) or with (std+) amines for 24 hours. However, we found that plating of HCECs on these nanofibrillar surfaces did not reduce TGF-ß2 mRNA levels (Fig. 6A) . HCECs were less spread and more rounded when plated on nanofibrillar surfaces versus plastic, reduced-Matrigel, or Aclar coverslips (Fig. 6B) . This suggests that the cells were responding to the 3-D matrix, as described previously for other cells types.36 The results do not support the idea that the 3-D topography of Matrigel is the controlling factor determining reduction in TGF-ß2 production.


Figure 6
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  		FIGURE 6. Basement membrane–like topology does not reduce TGF-ß2 mRNA levels in HCECs. HCECs were plated overnight in serum-free KSM at a density of 105 per well on a 12-well plastic plate (P), coated with laminin (LM) or GFR-Matrigel (rM), or on an Aclar coverslip (Aclar-none) or an Aclar coverslip electrospun with nanofibers linked without (Aclar-std) or with (Aclar-std+) amines. (A) Total RNA was harvested after 24 hours and subjected to qRT-PCR. The relative TGF-ß2 mRNA is calculated as a ratio of the TGF-ß2 to the loading control threshold cycles and represents triplicates (average ± SD) from one of three experiments. *P < 0.05, GFR-Matrigel versus plastic. (B) Representative micrographs of HCECs plated on different ECMs.

 
Effect of Matrigel on Levels of the Cytoskeleton-Associated Protein Ezrin
The results of the preceding experiments indicated that neither individual biochemical components nor 3-D structure alone was sufficient to mediate Matrigel’s ability to reduce production of TGF-ß2. A re-evaluation of these findings suggested the new hypothesis that complexity is a requirement (i.e., the multiple components of Matrigel must interact in the appropriate way as a 3-D basement membrane–like matrix to reduce TGF-ß2 production by corneal epithelial cells).

The protein called ezrin, which belongs to the ERM family, plays a role in establishing polarity of epithelial cells in tissues, such as the retinal pigment epithelium of the eye.40 It also plays a functional role in transmitting intracellular signals from epithelial cells attached to basement membrane ECM molecules,41 is involved in cell-substrate adhesion42 and takes part in regulating TGF-ß2 expression.43 Therefore, we considered it to be a good candidate for participating in the mechanisms regulating HCECs’ response to Matrigel. To investigate this possible role, we looked for differences in intracellular ezrin levels in HCECs plated overnight on laminin or GFR-Matrigel. Immunostaining showed that many HCECs plated on laminin stained positive for ERM, whereas there were fewer positive HCECs when cells were plated on GFR-Matrigel (Fig. 7A) . Cell counts revealed that there were 66% ± 6% ezrin-positive cells when plated on laminin versus 30% ± 2% ezrin-positive cells when plated on GFR-Matrigel. This difference is significant (P < 0.05). Using immunoblot analysis, we quantified total ezrin levels in HCECs plated on GFR-Matrigel versus laminin (Fig. 7B) . We found a significantly reduced level of ezrin in HCECs plated on Matrigel. These results are consistent with a possible role for ezrin in determining Matrigel’s ability to reduce TGF-ß2 production by corneal epithelial cells.


Figure 7
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  		FIGURE 7. Matrigel regulates ezrin levels in HCECs. The HCECs were plated overnight in serum-free medium at a density of 105 per well on a 24-well plastic plate coated with laminin (LM) or GFR-Matrigel (rM). (A) Cells were immunostained for ERM (ezrin). The ezrin antibody was omitted from the No Primary control. Green: positive staining; red: nuclei counterstained with propidium iodide. (B) Cytoplasmic lysates from HCECs were harvested and examined by immunoblot analysis for ERM (ezrin). Relative protein is a ratio of the ERM to ß-actin band densities and is compiled from the results of three independent experiments (average ± SD). Ezrin bands are 80 kDa, and ß-actin bands are 42 kDa, based on molecular size markers (not shown). *P < 0.05, GFR-Matrigel versus laminin.

 

   Discussion
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 Abstract
 Materials and Methods
 Results
 Discussion
References
 
Surgical procedures in cornea that result in penetration of the epithelial basement membrane and Bowman’s layer typically stimulate a fibrotic repair response that results in deposition of a hazy repair tissue, interfering with corneal clarity.8 Recently, our research group implicated epithelial TGF-ß2 as a key modulator of fibrotic repair in the mouse cornea. We also found that rabbit epithelial cells produce much less TGF-ß2 protein when plated on Matrigel, a complex basement membrane–like extracellular matrix extract.11 12 The goal of the present study was to explore this initial finding further to acquire information that might focus a pharmacologic development strategy.

To increase clinical relevance we moved into a human model, after determining that TGF-ß2 is also the prominent human corneal epithelial isoform. We show that the effects of Matrigel cannot be explained by growth factor contaminants, reduction in heparin sulfate proteoglycans has no effect, and pure forms of the major ECM components laminin and collagen IV cannot alone reproduce the effect. Experiments also failed to implicate inhibition of a constitutive TGF-ß2 autocrine feedback loop. Thus, we went on to consider the hypotheses that incorporates a requirement for complexity. TGF-ß2 production was not inhibited by plating cells on a synthetic nanofiber matrix with a 3-D topography similar to Matrigel, previously shown to activate Rac signaling. However Matrigel caused a reduction in ezrin, a member of the ERM family that plays a role in establishing polarity of epithelial cells in tissues through the Rho signaling pathway. These findings indicate that Matrigel inhibits TGF-ß2 gene expression and point to a mechanism requiring the complexity of Matrigel composition and structure.

Although not specifically investigated in this study, Matrigel may alter TGF-ß2 protein processing. Like TGF-ß1b,44 TGF-ß2 is secreted in an inactive form as a complex composed of mature TGF-ß2 covalently linked to a latency-associated protein associated with a latent TGF-ß binding protein (LTBP). Previous reports indicate that TGF-ß2 is secreted more effectively when associated with LTBP.45 We have preliminary qRT-PCR data indicating that matrix does not change the level of LTBP-1 mRNA in human corneal epithelial cells (data not shown). Therefore, cells plated on either laminin or Matrigel would be able to secrete TGF-ß2 in an inactive form.

Differences between the Rabbit and Human Cell Culture Models
In the human model, we found that the decrease in intracellular TGF-ß2 protein levels in cells plated on Matrigel takes several days, whereas we were able to see this difference within 24 hours in the rabbit model.12 The reason for this difference is likely to be a reflection of various differences between the cell culture methodologies rather than a species difference. Because we had an ample source of tissue for rabbit cell culture, we were able to isolate cells directly from the tissue for use in experiments. Alternatively, human cells could be obtained only from small pieces of human tissues discarded after surgery, and it was necessary to expand the number of cells in culture before use in experiments. Corneal epithelial cells clearly change to some degree when expanded in culture—for example, their secreted gelatinolytic metalloproteinase signature shifts toward higher levels of gelatinase A (unpublished observations, 1990). Nevertheless, the HCECs used in this study retained the keratin differentiation marker for epithelium, as well as the preference for TGF-ß2 expression over TGF-ß1 that we saw in the rabbit model. Another change made necessary by the requirement for expanding the number of cells was use of a low-calcium medium to enhance the rate of cell replication. To maintain cell homeostasis, we used this same medium for experiments, as opposed to the standard calcium medium used in our previous rabbit study. Either of these differences could contribute to greater TGF-ß2 protein stability and alter the time course by which Matrigel reduces the protein level. Indeed, there are many reports in the literature about regulation of TGF-ß protein stability and the central role of this parameter in determining the ultimate level of TGF-ß activity.46 47 We would not attempt to derive any conclusions about the relevance of this finding to the in vivo situation since the conditions are so different. Fortuitously, however, this longer time frame was useful for our ability to characterize the phenomenon as we were easily able to observe the earlier decrease in TGF-ß2 mRNA levels and transcriptional promoter activity, which would have been more compressed in time in the rabbit model.

Failure to Implicate an Autocrine TGF-ß2 Feedback Loop
TGF-ßs can upregulate activity of the TGF-ß genes in cells that produce them via a positive autocrine feedback loop.25 In fact, we have previously shown that much of the TGF-ß2 produced by rabbit corneal epithelial cells in culture is in the biologically active form,14 15 which suggests a way that Matrigel acts to inhibit TGF-ß2 production—by repressing this feedback loop. In fact, the Matrigel component collagen IV has been reported to bind and sequester TGF-ß2,34 providing a possible mechanism for this inhibition. Our finding that purified collagen IV alone was not able to inhibit TGF-ß2 production, however, did not support this possibility. Additional experiments performed in this study also failed to provide support. The presence of Matrigel failed to inhibit the capacity of exogenously added TGF-ß2 to activate Smad3 signaling and stimulate TGF-ß2 mRNA levels. A preliminary immunoblot analysis that we performed on conditioned media from the cells treated with exogenous TGF-ß2 and plated on either laminin or Matrigel displayed relatively equal amounts of recombinant TGF-ß2 (data not shown), supporting the idea that Matrigel does not selectively sequester TGF-ß2.

In fact, the process that is used to create GFR-Matrigel does not reduce levels of naturally occurring TGF-ß2. It could be argued that Matrigel is already saturated with TGF-ßs and cannot absorb more; thus, exogenous TGF-ß2 could act without restraint, but TGF-ß2 produced endogenously by corneal epithelial cells should also be able to escape from this absorption. However, the strongest evidence against the autocrine inhibition mechanism is that exogenous TGF-ß2 increases the levels of TGF-ß2 mRNA without affecting TGF-ß2 promoter activity. Because Matrigel decreases both TGF-ß2 mRNA levels and TGF-ß2 gene promoter activity, we infer that there are different mechanisms at play. For example, TGF-ß2 mRNA levels could be increased in the absence of transcription by increasing mRNA stability, a well-known TGF-ß regulatory mechanism.48

Evidence for Involvement of the Actin Cytoskeleton
In epithelial cells, the cortical actin cytoskeleton is a highly dynamic structure that controls the localization of protein complexes associated with the plasma membrane and the machinery that regulates the actin assembly (reviewed in Ref. 49 ). Reorganization of the actin cytoskeleton is linked to signaling via the Rho family of small GTPases (reviewed in Ref. 50 ). The epithelial basement membrane has a complex 3-D architecture, and much work has indicated that this nanotopography can influence organization of the cortical cytoskeleton in cells in culture.35 Growth of cells on 3-D nanofibrillar surfaces results in a preferential and sustained activation of the small GTPase Rac.37 Cell surface receptors can also transmit signals into a cell via structural changes that occur when they bind to their ECM ligands (reviewed in Ref. 51 ). The cytoplasmic face of cell contact sites comprises large macromolecular assemblies that link transmembrane cell adhesion molecules to the cytoskeleton. These assemblies are dynamic structures that are the targets of regulatory signals that control cell adhesiveness.52 The ERM family proteins are part of the cortical cytoskeleton. Immunofluorescence studies of cultured epithelial cells have revealed that ERM proteins are coexpressed and co-concentrated at cell-surface structures such as microvilli, filopodia, uropods, ruffling membranes, retraction fibers, and cell-adhesion sites where actin filaments are associated with plasma membranes.53 Signal transduction through ERM proteins has emerged as an important means of coordinating localized and dynamic cellular processes that require membrane cytoskeletal reorganization.49 54 They play an important role in the activation of members of the Rho family by recruiting their regulators.55 Our finding that levels of the ERM protein ezrin are regulated by plating of corneal epithelial cells on Matrigel suggests ERM proteins and the Rho pathway as a focus for future studies to understand how Matrigel controls TGF-ß2 production.

It seems a paradox that the complex basement membrane–like ECM Matrigel should inhibit TGF-ß2 production in cell culture, but that there should be so much TGF-ß2 protein present in the normal uninjured corneal epithelium—a previous finding12 now confirmed in this study. How can we understand the cell culture phenomenon in terms of corneal biology? Cell culture bears much in common with wound healing, and our previous findings have suggested that epithelial cells migrating over basement membrane to close a superficial corneal abrasion downregulate TGF-ß2 production, but cells migrating over a stromal wound bed upregulate TGF-ß2 production. Once the epithelium is completely repaired, however, TGF-ß2 synthesis may once again increase despite the presence of the basement membrane. Understanding basement membrane regulation of corneal epithelial TGF-ß2 as a cytoskeletal-regulated process involving the complexity of basement membrane structure and biochemical composition may help make sense of this paradox. Migrating cells have much different cytoskeletal organization and ECM adhesions than cells in the normal differentiated epithelium, and the associating regulatory proteins are different.56 It is in these differences that we are likely to find the answers to how basement membrane regulates TGF-ß2 production.

In the present study, our goal was to identify mechanisms by which Matrigel inhibits TGF-ß2 production. We show that TGF-ß2 protein production is controlled at multiple levels of gene expression by Matrigel, including protein accumulation, mRNA accumulation and activity of the gene’s transcriptional promoter. The effects of Matrigel cannot be explained by growth factor contaminants and cannot be reproduced by purified matrix components or by a structurally similar synthetic matrix that stimulates Rac signaling pathway. The capacity of Matrigel to reduce ezrin focuses future studies on the ERM/Rho signaling pathway.


   Acknowledgements
 
The authors thank Magda Celdran from the histology core for technical assistance; Darlene Miller from the clinical microbiology section and Sander Dubovy, MD, from the Florida Lions Eye Bank, Inc., for obtaining donor tissue; and Carmen A. Puliafito, MD, MBA, Department Chair, for overall support.


   Footnotes
 
Supported by National Eye Institute Grants EY009828 and EY014801 and also an unrestricted grant from Research to Prevent Blindness. MEF was a Research to Prevent Blindness Senior Scientific Investigator when this work was done and she holds the Walter G. Ross Chair in Ophthalmic Research.

Submitted for publication July 7, 2006; revised October 17, 2006; accepted January 11, 2007.

Disclosure: A.J. LaGier, None; S.H. Yoo, None; E.C. Alfonso, None; S. Meiner, Donaldson Co., Inc. (C); M.E. Fini, 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: M. Elizabeth Fini, Bascom Palmer Eye Institute, University of Miami, Miller School of Medicine, McKnight Vision Research Center, 1638 NW 10th Avenue, Miami, FL 33136; efini{at}med.miami.edu.


   References
Top
 Abstract
 Materials and Methods
 Results
 Discussion
 References
 

  1. Cintron C, Kublin CL. Regeneration of corneal tissue. Dev Biol. 1977;61:346–357.[CrossRef][ISI][Medline][Order article via Infotrieve]
  2. Fini ME. Keratocyte and fibroblast phenotypes in the repairing cornea. Prog Retin Eye Res. 1999;18:529–551.[CrossRef][ISI][Medline][Order article via Infotrieve]
  3. Grinnell F. Fibroblasts, myofibroblasts, and wound contraction. J Cell Biol. 1994;124:401–404.[Free Full Text]
  4. Weimar V. Healing Processes in the Cornea. 1960;111–124. Blackwell Scientific Publications Oxford, UK.
  5. Ferguson MW, O’Kane S. Scar-free healing: from embryonic mechanisms to adult therapeutic intervention. Philos Trans R Soc Lond B Biol Sci. 2004;359:839–850.[CrossRef][ISI][Medline][Order article via Infotrieve]
  6. Desmouliere A, Chaponnier C, Gabbiani G. Tissue repair, contraction, and the myofibroblast. Wound Repair Regen. 2005;13:7–12.[CrossRef][ISI][Medline][Order article via Infotrieve]
  7. Martin P. Wound healing: aiming for perfect skin regeneration. Science. 1997;276:75–81.[Abstract/Free Full Text]
  8. Møller-Pedersen T, Cavanagh HD, Petroll WM, Jester JV. Neutralizing antibody to TGFß modulates stromal fibrosis but not regression of photoablative effect following PRK. Curr Eye Res. 1998;17:736–747.[CrossRef][ISI][Medline][Order article via Infotrieve]
  9. Singer AJ, Clark RA. Cutaneous wound healing. N Engl J Med. 1999;341:738–746.[Free Full Text]
  10. Wilson SE, Mohan RR, Mohan RR, Ambrosio R, Jr, Hong J, Lee J. The corneal wound healing response: cytokine-mediated interaction of the epithelium, stroma, and inflammatory cells. Prog Retin Eye Res. 2001;20:625–637.[CrossRef][ISI][Medline][Order article via Infotrieve]
  11. Fini ME, Stramer BM. How the cornea heals: cornea-specific repair mechanisms impacting on surgical outcomes. Cornea. 2005;24(suppl 8)S2–S11.[CrossRef][ISI][Medline][Order article via Infotrieve]
  12. Stramer BM, Zieske JD, Jung JC, Austin JS, Fini ME. Molecular mechanisms controlling the fibrotic repair phenotype in cornea: implications for surgical outcomes. Invest Ophthalmol Vis Sci. 2003;44:4237–4246.[Abstract/Free Full Text]
  13. Klenkler B, Sheardown H. Growth factors in the anterior segment: role in tissue maintenance, wound healing and ocular pathology. Exp Eye Res. 2004;79:677–688.[CrossRef][ISI][Medline][Order article via Infotrieve]
  14. Strissel KJ, Rinehart WB, Fini ME. A corneal epithelial inhibitor of stromal cell collagenase synthesis identified as TGF-ß2. Invest Ophthalmol Vis Sci. 1995;36:151–162.[Abstract/Free Full Text]
  15. Strissel KJ, Rinehart WB, Fini ME. Regulation of paracrine cytokine balance controlling collagenase synthesis by corneal cells. Invest Ophthalmol Vis Sci. 1997;38:546–552.[Abstract/Free Full Text]
  16. Mead AL, Wong TT, Cordeiro MF, Anderson IK, Khaw PT. Evaluation of anti-TGF-ß2 antibody as a new postoperative anti-scarring agent in glaucoma surgery. Invest Ophthalmol Vis Sci. 2003;44:3394–3401.[Abstract/Free Full Text]
  17. Stramer BM, Austin JS, Roberts AB, Fini ME. Selective reduction of fibrotic markers in repairing corneas of mice deficient in Smad3. J Cell Physiol. 2005;203:226–232.[CrossRef][ISI][Medline][Order article via Infotrieve]
  18. Sobrin L, Liu Z, Monroy DC, et al. Regulation of MMP-9 activity in human tear fluid and corneal epithelial culture supernatant. Invest Ophthalmol Vis Sci. 2000;41:1703–1709.[Abstract/Free Full Text]
  19. Kruse FE, Tseng SC. Serum differentially modulates the clonal growth and differentiation of cultured limbal and corneal epithelium. Invest Ophthalmol Vis Sci. 1993;34:2976–2989.[Abstract/Free Full Text]
  20. Taub M, Wang Y, Szczesny TM, Kleinman HK. Epidermal growth factor or transforming growth factor alpha is required for kidney tubulogenesis in matrigel cultures in serum-free medium. Proc Natl Acad Sci USA. 1990;87:4002–4006.[Abstract/Free Full Text]
  21. Ahmed I, Liu HY, Mamiya PC, et al. Three-dimensional nanofibrillar surfaces covalently modified with tenascin-C-derived peptides enhance neuronal growth in vitro. J Biomed Mater Res A. 2006;76:851–860.[Medline][Order article via Infotrieve]
  22. Noma T, Glick AB, Geiser AG, et al. Molecular cloning and structure of the human transforming growth factor-ß2 gene promoter. Growth Factors. 1991;4:247–255.[Medline][Order article via Infotrieve]
  23. Brand T, Schneider MD. Inactive type II and type I receptors for TGFß are dominant inhibitors of TGFß-dependent transcription. J Biol Chem. 1995;270:8274–8284.[Abstract/Free Full Text]
  24. Hayashi K, Frangieh G, Wolf G, Kenyon KR. Expression of transforming growth factor-ß in wound healing of vitamin A-deficient rat corneas. Invest Ophthalmol Vis Sci. 1989;30:239–247.[Abstract/Free Full Text]
  25. Li DQ, Tseng SC. Three patterns of cytokine expression potentially involved in epithelial-fibroblast interactions of human ocular surface. J Cell Physiol. 1995;163:61–79.[CrossRef][ISI][Medline][Order article via Infotrieve]
  26. Nishida K, Sotozono C, Adachi W, Yamamoto S, Yokoi N, Kinoshita S. Transforming growth factor-ß1, -ß2 and -ß3 mRNA expression in human cornea. Curr Eye Res. 1995;14:235–241.[ISI][Medline][Order article via Infotrieve]
  27. Pasquale LR, Dorman-Pease ME, Lutty GA, Quigley HA, Jampel HD. Immunolocalization of TGF-ß1, TGF-ß2, and TGF-ß3 in the anterior segment of the human eye. Invest Ophthalmol Vis Sci. 1993;34:23–30.[Abstract/Free Full Text]
  28. Wilson SE, He YG, Lloyd SA. EGF, EGF receptor, basic FGF, TGF ß-1, and IL-1 alpha mRNA in human corneal epithelial cells and stromal fibroblasts. Invest Ophthalmol Vis Sci. 1992;33:1756–1765.[Abstract/Free Full Text]
  29. Wilson SE, Lloyd SA, He YG. EGF, basic FGF, and TGF ß-1 messenger RNA production in rabbit corneal epithelial cells. Invest Ophthalmol Vis Sci. 1992;33:1987–1995.[Abstract/Free Full Text]
  30. Wilson SE, Schultz GS, Chegini N, Weng J, He YG. Epidermal growth factor, transforming growth factor alpha, transforming growth factor ß, acidic fibroblast growth factor, basic fibroblast growth factor, and interleukin-1 proteins in the cornea. Exp Eye Res. 1994;59:63–71.[CrossRef][ISI][Medline][Order article via Infotrieve]
  31. Schermer A, Galvin S, Sun TT. Differentiation-related expression of a major 64K corneal keratin in vivo and in culture suggests limbal location of corneal epithelial stem cells. J Cell Biol. 1986;103:49–62.[Abstract/Free Full Text]
  32. Colvin RB. Fibronectin. 1989;213–252. Academic Press New York.
  33. Nabi IR, Mathews AP, Cohen-Gould L, Gundersen D, Rodriguez-Boulan E. Immortalization of polarized rat retinal pigment epithelium. J Cell Sci. 1993;104:37–49.[Abstract]
  34. Paralkar VM, Vukicevic S, Reddi AH. Transforming growth factor ß type 1 binds to collagen IV of basement membrane matrix: implications for development. Dev Biol. 1991;143:303–308.[CrossRef][ISI][Medline][Order article via Infotrieve]
  35. Schindler M, Nur EKA, Ahmed I, et al. Living in three dimensions: 3-D nanostructured environments for cell culture and regenerative medicine. Cell Biochem Biophys. 2006;45:215–228.[CrossRef][ISI][Medline][Order article via Infotrieve]
  36. Schindler M, Ahmed I, Kamal J, et al. A synthetic nanofibrillar matrix promotes in vivo-like organization and morphogenesis for cells in culture. Biomaterials. 2005;26:5624–5631.[CrossRef][ISI][Medline][Order article via Infotrieve]
  37. Nur EKA, Ahmed I, Kamal J, Schindler M, Meiners S. Three dimensional nanofibrillar surfaces induce activation of Rac. Biochem Biophys Res Commun. 2005;331:428–434.[CrossRef][ISI][Medline][Order article via Infotrieve]
  38. Bhowmick NA, Ghiassi M, Bakin A, et al. Transforming growth factor-ß1 mediates epithelial to mesenchymal transdifferentiation through a RhoA-dependent mechanism. Mol Biol Cell. 2001;12:27–36.[Abstract/Free Full Text]
  39. Wakefield LM, Roberts AB. TGF-ß signaling: positive and negative effects on tumorigenesis. Curr Opin Genet Dev. 2002;12:22–29.[CrossRef][ISI][Medline][Order article via Infotrieve]
  40. Bonilha VL, Finnemann SC, Rodriguez-Boulan E. Ezrin promotes morphogenesis of apical microvilli and basal infoldings in retinal pigment epithelium. J Cell Biol. 1999;147:1533–1548.[Abstract/Free Full Text]
  41. O’Toole EA, Marinkovich MP, Hoeffler WK, Furthmayr H, Woodley DT. Laminin-5 inhibits human keratinocyte migration. Exp Cell Res. 1997;233:330–339.[CrossRef][ISI][Medline][Order article via Infotrieve]
  42. Takeuchi K, Sato N, Kasahara H, et al. Perturbation of cell adhesion and microvilli formation by antisense oligonucleotides to ERM family members. J Cell Biol. 1994;125:1371–1384.[Abstract/Free Full Text]
  43. Wick W, Grimmel C, Wild-Bode C, Platten M, Arpin M, Weller M. Ezrin-dependent promotion of glioma cell clonogenicity, motility, and invasion mediated by BCL-2 and transforming growth factor-ß2. J Neurosci. 2001;21:3360–3368.[Abstract/Free Full Text]
  44. Wakefield LM, Smith DM, Flanders KC, Sporn MB. Latent transforming growth factor-ß from human platelets: a high molecular weight complex containing precursor sequences. J Biol Chem. 1988;263:7646–7654.[Abstract/Free Full Text]
  45. Miyazono K, Thyberg J, Heldin CH. Retention of the transforming growth factor-ß 1 precursor in the Golgi complex in a latent endoglycosidase H-sensitive form. J Biol Chem. 1992;267:5668–5675.[Abstract/Free Full Text]
  46. Miyazono K, Olofsson A, Colosetti P, Heldin CH. A role of the latent TGF-ß 1-binding protein in the assembly and secretion of TGF-ß 1. EMBO J. 1991;10:1091–1101.[ISI][Medline][Order article via Infotrieve]
  47. Wakefield LM, Winokur TS, Hollands RS, Christopherson K, Levinson AD, Sporn MB. Recombinant latent transforming growth factor ß1 has a longer plasma half-life in rats than active transforming growth factor ß1, and a different tissue distribution. J Clin Invest. 1990;86:1976–1984.[ISI][Medline][Order article via Infotrieve]
  48. Kim SJ, Park K, Koeller D, et al. Post-transcriptional regulation of the human transforming growth factor-ß1 gene. J Biol Chem. 1992;267:13702–13707.[Abstract/Free Full Text]
  49. Bretscher A, Reczek D, Berryman M. Ezrin: a protein requiring conformational activation to link microfilaments to the plasma membrane in the assembly of cell surface structures. J Cell Sci. 1997;110:3011–3018.[Abstract]
  50. Hall A. Rho GTPases and the actin cytoskeleton. Science. 1998;279:509–514.[Abstract/Free Full Text]
  51. Calderwood DA, Shattil SJ, Ginsberg MH. Integrins and actin filaments: reciprocal regulation of cell adhesion and signaling.