|Molecular Vision 2004;
Received 30 July 2003 | Accepted 7 January 2004 | Published 15 January 2004
Diverse NF-κB expression in epiretinal membranes after human diabetic retinopathy and proliferative vitreoretinopathy
Takayuki Harada,1,2,3 Yoshinori
Mitamura,5,6 Hun-Meng A. Quah,1 Kenji Ohtsuka,5
Satoshi Kotake,4 Shigeaki Ohno,4 Keiji Wada,2 Shinobu
Takeuchi,6 Kohichi Tanaka1,7
1Laboratory of Molecular Neuroscience, School of Biomedical Science and Medical Research Institute, Tokyo Medical and Dental University, Tokyo, Japan; 2Department of Degenerative Neurological Diseases, National Institute of Neuroscience, National Center of Neurology and Psychiatry, Kodaira, Tokyo, Japan; 3Department of Molecular Neurobiology, Tokyo Metropolitan Institute for Neuroscience, Fuchu, Tokyo, Japan; 4Department of Ophthalmology and Visual Sciences, Hokkaido University Graduate School of Medicine, Sapporo, Hokkaido, Japan; 5Department of Ophthalmology, Sapporo Medical University School of Medicine, Sapporo, Hokkaido, Japan; 6Department of Ophthalmology, Toho University Sakura Hospital, Sakura, Chiba, Japan; 7PRESTO, Japan Science and Technology Corporation (JST), Kawaguchi, Saitama, Japan
Correspondence to: Takayuki Harada, M.D., Ph.D., Department of Molecular Neurobiology, Tokyo Metropolitan Institute for Neuroscience, 2-6 Musashidai, Fuchu, Tokyo 183-8526, Japan; Phone: +81-42-325-3881; FAX: +81-42-321-8678; email: firstname.lastname@example.org
Purpose: Formation of epiretinal membranes (ERMs) after proliferative diabetic retinopathy (PDR) and proliferative vitreoretinopathy (PVR) results in progressive deterioration of vision, but its pathogenic mechanisms are still unknown. This study was conducted to examine the role of nuclear factor kappa B (NF-κB) in the formation of ERMs after PDR and PVR.
Methods: ERM samples were obtained by vitrectomy from 10 patients with PDR (aged 53±12 years with 14±5 years of diabetes), 20 patients with PVR, and 17 patients with idiopathic ERMs. Ten PVR and 17 idiopathic ERM samples were processed for reverse transcription-polymerase chain reaction (RT-PCR) analysis. In addition, 10 PDR and 10 PVR membranes were processed for immunohistochemical analysis.
Results: NF-κB mRNA expression levels were significantly higher (10 of 10 versus 9 of 17 subjects in idiopathic ERM, p=0.0119) in PVR subjects. Immunohistochemical analysis showed NF-κB protein expression in 8 of the 10 PDR samples as well as all 10 PVR samples, and NF-κB positive cells were partially double labeled with glial cell markers. Interestingly, NF-κB protein was also overlapped with angiogenic factor interleukin-8 (IL-8) in glial cells as well as vascular endothelial cells.
Conclusions: These results suggest that NF-κB is involved in the formation of both glial and vascular endothelial cell components, and that these two cell types might have functional interactions that lead to the enlargement of intraocular proliferative membranes.
Epiretinal membranes (ERMs) involving the macular or perimacular regions can cause a reduction in vision, metamorphopsia, micropsia, or occasionally monocular diplopia. The presence of ERMs has been associated with various clinical conditions including proliferative diabetic retinopathy (PDR) and proliferative vitreoretinopathy (PVR) . The prevalence of ERMs in PDR is reported to be about 20% in Type 1 diabetes and about 5% in Type 2 diabetes [2,3]. PVR occurs when traction-generating cellular membranes develop in the vitreous and inner or outer surfaces of the retina after retinal detachment or major ocular trauma, and is the most common cause of failed repair of retinal detachment [4,5]. In general, PVR is considered to be a proliferative vitreoretinal disorder that is not related to retinal neovascularization. However, previous studies indicate that some PVR membranes were accompanied by a vascular component . ERMs after PDR and PVR are composed of many cell types such as glial cells, retinal pigment epithelial cells, and vascular endothelial cells [6-8], but their pathogenic mechanisms are still unknown. However, various trophic factors and cytokines, such as basic fibroblast growth factor (bFGF), vascular endothelial cell growth factor (VEGF), and interleukin-8 (IL-8) were detected in vitreous fluid and ERM samples derived from PDR and PVR patients, and they are presumed to be involved in the pathogenesis of proliferative membranes [9-12].
In a previous study, we examined the expression of various neurotrophic factor receptors in ERMs following PDR, and found high expression levels of glial cell line-derived neurotrophic factor (GDNF) receptors . GDNF family members mediate their actions through a multicomponent receptor complex composed of a transmembrane tyrosine kinase receptor, Ret, and one of the four glycosyl-phosphatidyl inositol (GPI)-linked GDNF family receptor α, designated GFRα1-GFRα4 . Among them, GFRα2 mRNA was detected in 89% of PDR membranes, and GFRα2 protein was mainly observed in the glial cell component . On the other hand, nuclear factor kappa B (NF-κB) p50 mRNA was detected in 91% of PDR membranes, and the active form of NF-κB p50 protein was observed in various cell populations . However, we examined only the vascular endothelial cells, forsaking all other cell populations that were NF-κB positive. NF-κB is a transcription factor that can be activated by hypoxia, bacteria, viral proteins, various cytokines and trophic factors including tumor necrosis factor-α (TNF-α), interleukin-1β, and GDNF [16-18]. Interestingly, NF-κB is activated within 3 days after retinal detachment, in a time frame consistent with its potential for contributing to secondary cellular changes . These results suggest the possibility that NF-κB, in combination with GDNF receptors, may be involved in the formation of the glial cell component of ERMs after PDR and PVR [15,18,20,21]. In addition, NF-κB expression in PVR membranes has yet to be examined.
In this study, we determined the coexpression of NF-κB p50 and GFRα2 proteins in PVR as well as PDR subjects. In addition, we found that NF-κB protein is overlapped with angiogenic factor interleukin-8 (IL-8) in both glial and vascular endothelial cells. We also proposed possible glia-vascular endothelial cell interactions in proliferative membranes.
This study was carried out in accordance with the tenets of the Helsinki Declaration. Informed consent was obtained from each patient for the collection of samples. Criteria for inclusion in the study were less than 80 years old, absence of renal or hematological diseases or uremia, absent administration of chemotherapy or life-support measures, and the fewest possible chronic pathologies other than diabetes. All PVR cases were grade C2 or worse according to the classification recommended by the Retina Society Terminology Committee . The epiretinal membranes were surgically removed from consecutive eyes with secondary ERM after PDR (10 eyes) and PVR (20 eyes) or idiopathic ERM (controls, 17 eyes) undergoing pars plana vitrectomy and membrane peeling at Toho University Sakura Hospital. Membranes were dissected from the retinal surface with horizontal scissors or membrane pick. Samples derived from 10 of the PVR patients (age 45±23 years) and 17 control subjects (age 67±8 years) were processed for reverse transcription-polymerase chain reaction (RT-PCR) analysis. The remainder of the PVR samples (from subjects aged 43±17 years) and PDR samples (from subjects aged 53±12 years, duration of diabetes 14 ±5 years) were processed for immunohistochemistry. These samples were embedded in optimum cutting temperature (OCT) compound (Miles Laboratories, Naperile, IL), flash-frozen in liquid nitrogen, and then stored at -80 °C.
RNA extraction and amplification by RT-PCR
Total cellular RNA was prepared as previously reported [13,15]. RNA (0.1 μg) extracted from each sample was reverse transcribed into first-strand cDNA using the Superscript Preamplification System (Gibco, Paisley, Scotland) and oligo-dT primers.
RT-PCR analysis was carried out as previously described [13,23]. Complementary DNA reverse transcribed from total RNA was amplified by using primers specific for human NF-κB p50 (sense: 5'-CAC TTA TGG ACA ACT ATG AGG TCT CTG G-3'; antisense: 5'-CTG TCT TGT GGA CAA CGC AGT GGA ATT TTA GG-3'), GFRα1 (sense: 5'-AAG CAC AGC TAC GGG ATG CT-3'; antisense: 5'-GGT CAC ATC TGA GCC ATT GC-3'), GFRα2 (sense: 5'-ACG AGA CCC TCC GCT CTT TG-3'; antisense: 5'-GGG AGG CTT CGT AGA ACT CCT C-3'), and Ret (sense: 5'-TGG CAA TTG AAT CCC TTT TT-3'; antisense: 5'-ATG CCA TAG AGT TTG TTT TC-3'). PCR was done after initial denaturation at 94 °C for 3 min. Each cycle consisted of a heat-denaturation step at 94 °C for 15 s, annealing of primers at either 58 °C (GFRα2), 60 °C (GFRα1 and Ret), or 61 °C (NF-κB p50) for 2 min, followed by polymerization at 72 °C for 2 min. The expected sizes of the amplified cDNA fragments of NF-κB p50, GFRα1, GFRα2, and Ret were 406, 441, 339, and 439 bp, respectively. Human cDNA acquired from testis (Takara, Kyoto, Japan) was used as a positive control. Negative controls for PCR were made using "templates" derived from reverse transcription reactions lacking either reverse transcriptase or total RNA. After 35 cycles, 15 μl of each reaction mixture was electrophoresed on a 2% Tris borate-EDTA agarose gel and stained with ethidium bromide.
Frozen sections (7 μm thick) were cut by a cryostat, mounted on 3-aminopropyltriethoxysilane coated glass slides, and air-dried at room temperature. For immunohistochemical analysis, the sections were fixed in ice cold acetone and then washed with phosphate buffered saline (PBS). The sections were incubated with normal donkey serum for 30 min to block non-specific staining. They were incubated overnight at 4 °C with an affinity-purified rabbit polyclonal antibody raised against amino acids 350 to 363 mapping within the nuclear location signal (NLS) region of human NF-κB p50  (2.0 μg/ml; Santa Cruz Biotechnology, Santa Cruz, CA). For double labeling immunofluorescence studies, they were then incubated with a goat polyclonal antibody against GFRα2 (1.0 μg/ml; Santa Cruz Biotechnology), a mouse monoclonal antibody against vimentin (1x; Zymed, San Francisco, CA), GFAP (50x; DAKO, Glostrup, Denmark), glutamine synthetase (1.0 μg/ml; Chemicon, Temecula, CA)  or IL-8 (1.0 μg/ml; Santa Cruz Biotechnology). NF-κB p50 was visualized with FITC-conjugated donkey anti-rabbit IgG (200x; Jackson Immunoresearch, West Groove, PA) while GFRα2 and GFAP were visualized with Cy3-conjugated donkey anti-goat or anti-mouse IgG (800x; Jackson Immunoresearch), respectively. In the case of vimentin, glutamine synthetase and IL-8 which were visualized with FITC-conjugated donkey anti-mouse IgG (200x; Jackson Immunoresearch), NF-κB p50 was visualized with Cy3-conjugated donkey anti-rabbit IgG (1000x; Amersham Pharmacia Biotech, Piscataway, NJ). For double labeling immunofluorescence study of IL-8 and GFAP, the sections were incubated with a mouse monoclonal antibody against IL-8 (1.0 μg/ml; Santa Cruz Biotechnology) and a rabbit polyclonal antibody against GFAP (500x; DAKO). IL-8 was visualized with FITC-conjugated donkey anti-mouse IgG (200x; Jackson Immunoresearch) while GFAP was visualized with Cy3-conjugated donkey anti-rabbit IgG (1000x; Amersham Pharmacia Biotech). The sections were examined by a confocal laser scanning microscope (Olympus, Tokyo, Japan). Primary antibody preabsorbed by blocking peptide (Santa Cruz Biotechnology) was used for negative controls. The adjacent section of each specimen was stained with 4,6-diamidino-2-phenylindole (DAPI).
Data are presented as mean±SEM except as noted. The χ2 test was used to test for significance of the difference between presence of various mRNAs examined in PVR versus controls. Statistical significance was accepted at p<0.05.
Expression of NF-κB p50 and GDNF receptors in ERMs after PVR was examined by RT-PCR analysis. As shown in Table 1, NF-κB p50 mRNA was detected in all 10 (100%) PVR patients, but in 9 of 17 (53%) idiopathic ERM (control) patients (a statistically significant difference in p50 mRNA expression between PVR and control patients; p=0.0119). GFRα1 mRNA was detected in 14 of 17 (82%) control subjects, but in 4 of 10 (40%) PVR patients (p=0.0393). On the other hand, GFRα2 mRNA was detected in 6 of 10 (60%) PVR patients, but in only 2 of 17 (12%) control subjects (p=0.0248). Ret mRNA was detected in 3 of 10 (30%) PVR patients and 6 of 17 (35%) controls (p>0.9999). We also examined the relationship between NF-κB p50 and GFRα mRNA expressions in both PVR and control patients (Table 1). NF-κB positive and GFRα1 positive patients were found in 4 of 10 (40%) of those with PVR, and 8 of 17 (47%) control subjects. On the other hand, NF-κB positive and GFRα2 positive patients were found in 6 of 10 (60%) PVR subjects, but only 1 of 17 (6%) control patients.
Immunohistochemical analysis was performed to identify the activated form of NF-κB p50 and GFRα2 protein expressions in ERMs after PVR. NF-κB protein was detected in all 10 samples examined (Figure 1A,B), and many NF-κB positive cells were double labeled with GFRα2 (yellow in Figure 1A). Since GFRα2 protein expression is increased in the glial component of ERMs after PDR, we examined whether NF-κB is coexpressed with a glial cell marker, vimentin . PVR membranes contained many glial cells, and some of them were double labeled with NF-κB (yellow in Figure 1B). Similar results were obtained in experiments using other glial cell markers such as glutamine synthetase or GFAP (data not shown). NF-κB or GFRα2 immunoreactivity was completely abolished when the primary antibody was preabsorbed with blocking peptide (data not shown).
We previously demonstrated that NF-κB p50 mRNA is expressed in 20 of 22 ERMs derived from PDR patients (91%) , but did not examine whether its protein is distributed to glial cells like PVR membranes (Figure 1). To examine this possibility, we carried out double labeling immunohistochemistry for the activated form of NF-κB p50 protein and glial cell markers. NF-κB protein was detected in 8 of 10 PDR subjects examined, and many NF-κB positive cells were double labeled with GFAP (arrowheads in Figure 2A) as well as GFRα2 (arrowheads in Figure 2B). Similar results were obtained in experiments using other glial cell markers such as glutamine synthetase or vimentin (data not shown). NF-κB or GFRα2 immunoreactivity was completely abolished when the primary antibody was preabsorbed with blocking peptide (data not shown).
Previous studies have shown that IL-8 induced by NF-κB plays a key role in retinal angiogenesis after PDR . In addition, we recently found that IL-8 is expressed in the neovascular component of PDR membranes, but did not examine its expression in other cell types . Since NF-κB is expressed in glial cells (Figure 2A), we examined whether IL-8 protein is also distributed to the glial cell region. Interestingly, IL-8 (Figure 3A) and GFAP (Figure 3B) proteins are partially overlapped in PDR membranes (yellow in Figure 3C). Such IL-8 immunoreactivity was completely abolished when the primary antibody was preabsorbed with blocking peptide for IL-8 (data not shown). These results suggest a possibility that IL-8 protein might be produced in glial cells in PDR membranes. Similar results were also observed in PVR membranes (data not shown).
This study shows high expression levels of NF-κB and GFRα2 mRNAs in ERMs after PVR as well as PDR . In addition, NF-κB and GFRα2 or angiogenic factor IL-8 proteins were coexpressed in glial cells in both PDR and PVR membranes. Together with our previous findings that NF-κB is expressed in vascular endothelial cells , NF-κB might be involved in the formation of both glial and neovascular components. On the other hand, glial cells can produce and secrete several factors that stimulate the proliferation of other cell types in ERMs [26-29]. Thus, inhibition of NF-κB activation and IL-8 production in glial cells may modify glia-vascular cell interactions and prevent the formation and enlargement of proliferative membranes. We have suggested a similar concept in the case of retinal degeneration [28,29].
GDNF and neurturin are structurally-related and distant members of the transforming growth factor-β (TGF-β) superfamily . Recent studies have shown that TGF-β upregulates its own gene expression as well as genes that code for other polypeptide growth factors, such as interleukin-1 and bFGF, which are crucial for wound healing . In addition, we recently found that exogenous GDNF increases brain-derived neurotrophic factor (BDNF), bFGF, and GDNF productions in retinal Müller glial cells [29,31]. Since these factors are secreted from retinal injury sites, one possible cause of ERM formation after ocular trauma and vitreoretinal surgery is the increase in release and concentration of these growth factors. In this context, PVR membranes can be considered as an "over-healing" disease. On the other hand, PVR is characterized by a breakdown of the blood-retinal barrier (BRB) . Igarashi et al. recently demonstrated that barrier function of the BRB is regulated by GDNF and neurturin secreted from glial cells . These results suggest functional implications of GDNF, neurturin, and their receptors in both the initiation and the process of PVR membrane formation. Although GDNF might induce NF-κB activation , NF-κB positive cells in PVR and PDR samples are not always GFRα2 positive (Figure 1A and Figure 2B). In addition, NF-κB and GDNF receptor expressions were also detected in some idiopathic ERM samples (Table 1). Thus, the role of NF-κB and GFRα2 in the process of ERM formation should be determined in more detail. For example, quantitative analysis of these genes may support our present results. We are currently planning to use real-time PCR analysis and examine their roles in secondary ERMs after various diseases other than PDR and PVR.
Our present findings suggest the possibility that inhibiting biological activity of NF-κB and/or GFRα2 in the glial component may be useful in preventing the formation of intraocular proliferative membranes. Recent studies have shown that transfection of IκB mutant, which blocks NF-κB activation , can inhibit angiogenesis by suppressing the production of IL-8 [34,35]. Thus, utilizing angiogenic factor blockers in combination with NF-κB-specific blocker and/or antisence oligonucleotide could lead to possible synergistic inhibition of the formation of intraocular proliferative membranes. However, before determining this possibility, further investigations into the precise role of NF-κB on retinal cells and all cell types in ERMs will be needed.
Supported by Ministry of Education, Culture, Sports, Science and Technology of Japan; Ministry of Health, Labour and Welfare of Japan; Japan Foundation for Aging and Health; Japan Society for the Promotion of Science for Young Scientists (CH), and Japan Diabetes Foundation (TH).
1. Margherio RR, Margherio AR. Epiretinal macular membranes. In: Albert DM, Jakobiec FA, Azar DT, Gragoudas ES, editors. Principles and practice of ophthalmology. 2nd ed. Vol 6. Philadelphia:Saunders; 2000. p. 2103.
2. Klein R, Klein BE, Moss SE, Davis MD, DeMets DL. The Wisconsin epidemiologic study of diabetic retinopathy. II. Prevalence and risk of diabetic retinopathy when age at diagnosis is less than 30 years. Arch Ophthalmol 1984; 102:520-6.
3. Klein R, Klein BE, Moss SE, Davis MD, DeMets DL. The Wisconsin epidemiologic study of diabetic retinopathy. III. Prevalence and risk of diabetic retinopathy when age at diagnosis is 30 or more years. Arch Ophthalmol 1984; 102:527-32.
4. Cardillo JA, Stout JT, LaBree L, Azen SP, Omphroy L, Cui JZ, Kimura H, Hinton DR, Ryan SJ. Post-traumatic proliferative vitreoretinopathy. The epidemiologic profile, onset, risk factors, and visual outcome. Ophthalmology 1997; 104:1166-73.
5. Cowley M, Conway BP, Campochiaro PA, Kaiser D, Gaskin H. Clinical risk factors for proliferative vitreoretinopathy. Arch Ophthalmol 1989; 107:1147-51.
6. Asiyo-Vogel MN, El-Hifnawi ES, Bopp S, Laqua H. The vascular component of proliferative vitreoretinopathy membranes: an immunohistochemical and ultrastructural study. Retina 1998; 18:56-61.
7. Baudouin C, Fredj-Reygrobellet D, Baudouin F, Lapalus P, Gastaud P. Immunohistologic study of proliferative vitreoretinopathy. Am J Ophthalmol 1989; 108:387-94.
8. Weller M, Esser P, Heimann K, Wiedemann P. Retinal microglia: a new cell in idiopathic proliferative vitreoretinopathy? Exp Eye Res 1991; 53:275-81.
9. Wiedemann P. Growth factors in retinal diseases: proliferative vitreoretinopathy, proliferative diabetic retinopathy, and retinal degeneration. Surv Ophthalmol 1992; 36:373-84.
10. El-Ghrably IA, Dua HS, Orr GM, Fischer D, Tighe PJ. Detection of cytokine mRNA production in infiltrating cells in proliferative vitreoretinopathy using reverse transcription polymerase chain reaction. Br J Ophthalmol 1999; 83:1296-9.
11. Limb GA, Alam A, Earley O, Green W, Chignell AH, Dumonde DC. Distribution of cytokine proteins within epiretinal membranes in proliferative vitreoretinopathy. Curr Eye Res 1994; 13:791-8.
12. Mitamura Y, Takeuchi S, Matsuda A, Tagawa Y, Mizue Y, Nishihira J. Hepatocyte growth factor levels in the vitreous of patients with proliferative vitreoretinopathy. Am J Ophthalmol 2000; 129:678-80.
13. Harada T, Harada C, Mitamura Y, Akazawa C, Ohtsuka K, Ohno S, Takeuchi S, Wada K. Neurotrophic factor receptors in epiretinal membranes after human diabetic retinopathy. Diabetes Care 2002; 25:1060-5.
14. Baloh RH, Enomoto H, Johnson EM Jr, Milbrandt J. The GDNF family ligands and receptors - implications for neural development. Curr Opin Neurobiol 2000; 10:103-10.
15. Mitamura Y, Harada T, Harada C, Ohtsuka K, Kotake S, Ohno S, Tanaka K, Takeuchi S, Wada K. NF-kappaB in epiretinal membranes after human diabetic retinopathy. Diabetologia 2003; 46:699-703.
16. Hayashi H, Ichihara M, Iwashita T, Murakami H, Shimono Y, Kawai K, Kurokawa K, Murakumo Y, Imai T, Funahashi H, Nakao A, Takahashi M. Characterization of intracellular signals via tyrosine 1062 in RET activated by glial cell line-derived neurotrophic factor. Oncogene 2000; 19:4469-75.
17. Baeuerle PA, Henkel T. Function and activation of NF-kappaB in the immune system. Annu Rev Immunol 1994; 12:141-79.
18. Wang XC, Jobin C, Allen JB, Roberts WL, Jaffe GJ. Suppression of NF-kappaB-dependent proinflammatory gene expression in human RPE cells by a proteasome inhibitor. Invest Ophthalmol Vis Sci 1999; 40:477-86.
19. Geller SF, Lewis GP, Fisher SK. FGFR1, signaling, and AP-1 expression after retinal detachment: reactive Muller and RPE cells. Invest Ophthalmol Vis Sci 2001; 42:1363-9.
20. Yoshida A, Yoshida S, Hata Y, Khalil AK, Ishibashi T, Inomata H. The role of NF-kappaB in retinal neovascularization in the rat. Possible involvement of cytokine-induced neutrophil chemoattractant (CINC), a member of the interleukin-8 family. J Histochem Cytochem 1998; 46:429-36.
21. Yoshida A, Yoshida S, Khalil AK, Ishibashi T, Inomata H. Role of NF-kappaB-mediated interleukin-8 expression in intraocular neovascularization. Invest Ophthalmol Vis Sci 1998; 39:1097-106.
22. The Retina Society Terminology Committee. The classification of retinal detachment with proliferative vitreoretinopathy. Ophthalmology 1983; 90:121-5.
23. Harada T, Harada C, Sekiguchi M, Wada K. Light-induced retinal degeneration suppresses developmental progression of flip-to-flop alternative splicing in GluR1. J Neurosci 1998; 18:3336-43.
24. Hammes HP, Hoerauf H, Alt A, Schleicher E, Clausen JT, Bretzel RG, Laqua H. N(epsilon)(carboxymethyl)lysin and the AGE receptor RAGE colocalize in age-related macular degeneration. Invest Ophthalmol Vis Sci 1999; 40:1855-9.
25. Harada T, Harada C, Watanabe M, Inoue Y, Sakagawa T, Nakayama N, Sasaki S, Okuyama S, Watase K, Wada K, Tanaka K. Functions of the two glutamate transporters GLAST and GLT-1 in the retina. Proc Natl Acad Sci U S A 1998; 95:4663-6.
26. Amin RH, Frank RN, Kennedy A, Eliott D, Puklin JE, Abrams GW. Vascular endothelial growth factor is present in glial cells of the retina and optic nerve of human subjects with nonproliferative diabetic retinopathy. Invest Ophthalmol Vis Sci 1997; 38:36-47.
27. Behzadian MA, Wang XL, Shabrawey M, Caldwell RB. Effects of hypoxia on glial cell expression of angiogenesis-regulating factors VEGF and TGF-beta. Glia 1998; 24:216-25.
28. Harada T, Harada C, Nakayama N, Okuyama S, Yoshida K, Kohsaka S, Matsuda H, Wada K. Modification of glial-neuronal cell interactions prevents photoreceptor apoptosis during light-induced retinal degeneration. Neuron 2000; 26:533-41.
29. Harada T, Harada C, Kohsaka S, Wada E, Yoshida K, Ohno S, Mamada H, Tanaka K, Parada LF, Wada K. Microglia-Muller glia cell interactions control neurotrophic factor production during light-induced retinal degeneration. J Neurosci 2002; 22:9228-36.
30. Wong H, Wahl S. Inflammation and repair. In: Sporn MB, Roberts AB, editors. Handbook of experimental pharmacology. Berlin: Splinger-Verlag 1990; 95:509-48.
31. Harada C, Harada T, Quah HM, Maekawa F, Yoshida K, Ohno S, Wada K, Parada LF, Tanaka K. Potential role of glial cell line-derived neurotrophic factor receptors in Muller glial cells during light-induced retinal degeneration. Neuroscience 2003; 122:229-35.
32. Igarashi Y, Chiba H, Utsumi H, Miyajima H, Ishizaki T, Gotoh T, Kuwahara K, Tobioka H, Satoh M, Mori M, Sawada N. Expression of receptors for glial cell line-derived neurotrophic factor (GDNF) and neurturin in the inner blood-retinal barrier of rats. Cell Struct Funct 2000; 25:237-41.
33. Van Antwerp DJ, Martin SJ, Kafri T, Green DR, Verma IM. Suppression of TNF-alpha-induced apoptosis by NF-kappaB. Science 1996; 274:787-9.
34. Huang S, Robinson JB, Deguzman A, Bucana CD, Fidler IJ. Blockade of nuclear factor-kappaB signaling inhibits angiogenesis and tumorigenicity of human ovarian cancer cells by suppressing expression of vascular endothelial growth factor and interleukin 8. Cancer Res 2000; 60:5334-9.
35. Oitzinger W, Hofer-Warbinek R, Schmid JA, Koshelnick Y, Binder BR, de Martin R. Adenovirus-mediated expression of a mutant IkappaB kinase 2 inhibits the response of endothelial cells to inflammatory stimuli. Blood 2001; 97:1611-7.