High glucose-induced hyperosmolarity contributes to COX-2 expression and angiogenesis: implications for diabetic retinopathy
© Madonna et al. 2016
Received: 9 November 2015
Accepted: 22 January 2016
Published: 29 January 2016
We tested the hypothesis that glucose-induced hyperosmolarity, occurring in diabetic hyperglycemia, promotes retinal angiogenesis, and that interference with osmolarity signaling ameliorates excessive angiogenesis and retinopathy in vitro and in vivo.
Methods and Results
We incubated human aortic (HAECs) and dermal microvascular endothelial cells (HMVECs) with glucose or mannitol for 24 h and tested them for protein levels and in vitro angiogenesis. We used the Ins2 Akita mice as a model of type 1 diabetes to test the in vivo relevance of in vitro observations. Compared to incubations with normal (5 mmol/L) glucose concentrations, cells exposed to both high glucose and high mannitol (at 30.5 or 50.5 mmol/L) increased expression of the water channel aquaporin-1 (AQP1) and cyclooxygenase (COX)-2. This was preceded by increased activity of the osmolarity-sensitive transcription factor Tonicity enhancer binding protein (TonEBP), and enhanced endothelial migration and tubulization in Matrigel, reverted by treatment with AQP1 and TonEBP siRNA. Retinas of Ins2 Akita mice showed increased levels of AQP1 and COX-2, as well as angiogenesis, all reverted by AQP1 siRNA intravitreal injections.
Glucose-related hyperosmolarity seems to be able to promote angiogenesis and retinopathy through activation of TonEBP and possibly increasing expression of AQP1 and COX-2. Osmolarity signaling may be a target for therapy.
KeywordsGlucose Diabetes Hyperosmolarity Cyclooxygenase-2 Angiogenesis Microangiopathy Diabetic retinopathy
Hyperglycemia can cause diabetic micro-  and macrovascular complications  by triggering oxidative stress [3, 4], forming advanced glycation end products (AGEs) [4, 5], increasing the flux of glucose to sorbitol through the polyol and hexosamine pathways , activating protein kinase C (PKC) , and provoking inflammation  (reviewed in ). Diabetic microvascular disease is pathologically characterized by excessive vessel growth and increased vessel permeability [9, 10].
Hyperglycemia has been reported to increase the endothelial expression of the proinflammatory proteins intercellular adhesion molecule (ICAM)-1 and vascular cell adhesion molecule (VCAM)-1, and to decrease production of nitric oxide, all through activation of the water channel protein aquaporin (AQP)1 . Hyperosmotic stress inevitably accompanies hyperglycemia, and may therefore contribute to some aspects of hyperglycemia-induced vascular injury.
Similarly to VCAM-1 and ICAM-1, cyclooxygenase (COX)-2 participates in inflammation  and angiogenesis [13, 14]. Induced by cytokines, mitogens and endotoxin , COX-2 regulates the expression and activity of matrix metalloproteinase (MMP)-9 , which degrades extracellular matrix and promotes endothelial cell migration and vessel sprouting . Endothelial COX-2 has been implicated in angiogenesis (mostly in the context of tumorigenesis, reviewed in ), as well as in proliferative diabetic retinopathy , characterized by excessive angiogenesis [19–21]. COX-2 is expressed in human monocytes and macrophages, as well as human endothelial cells  exposed to high glucose .
Against this background, we therefore examined whether hyperosmotic stress, at levels attainable in diabetes, induces COX-2 expression in human micro- and macrovascular endothelial cells. We then analyzed the functional impact of hyperosmotic stress and COX-2 expression on angiogenesis and explored underlying mechanisms, particularly with regard to the involvement of water channels and associated signaling molecules. Finally, we investigated the in vivo implications of such findings for diabetic retinopathy in a mouse model.
d-glucose, D-mannitol and l-glucose (these two latter devoid of metabolic activities and used as a purely hyperosmolar controls), saccharose, and sodium chloride, were purchased from Sigma (St. Louis, MO, USA). The selective COX-2 inhibitor NS-398 was purchased from Calbiochem (Gibbstown, NJ, USA).
Male C57BL/6 mice (body weight: 15 ± 4 g, age: 1 year; n = 21) and male D2.B6-Ins2 Akita diabetic mice, a model of type 1 diabetes developing retinal angiogenesis [23, 24] (body weight: 11 ± 2 g, n = 21) were purchased from The Jackson Laboratories (Bar Harbor, ME, USA). All procedures were approved by our Institutional Ethics Committee for Animal Research. Investigations conformed to the Principles of Laboratory Animal Care formulated by the National Society for Medical Research and the Guide for the Care and Use of Laboratory Animals [NIH Publication 86–23, 1985 revision].
Subconfluent human aortic endothelial cells (HAECs) and human microvascular endothelial cells (HMVECs) at passage 3 were synchronized by starvation in Endothelial Basal Medium (EBM, Clonetics, Baltimore, MD, USA) for 24 h, then incubated with control d-glucose concentration (5.5 mmol/L, control and 285 mOsm/L), high glucose (HG: 30.5 mmol/L and 385 mOsm/L or 50.5 mmol/L and 460 mOsm/L), high mannitol (HM: 5.5 mmol/L glucose + 25 mmol/L and 385 mOsm/L or 45 mmol/L mannitol and 385 mOsm/L), for 24 or 72 h. In some experiments, cells were also incubated with l-glucose at equimolar concentrations, saccharose or sodium chloride, as further osmotic controls, in the presence or absence of 1–10 μg/mL NS-398.
Cell viability after treatments was assessed by cell morphology and cell count at phase-contrast microscopy, Trypan blue exclusion, and total protein content.
Total proteins from retinas of wild-type C57BL/6 male mice and sex/age matched D2.B6-Ins2 Akita diabetic mice, or from HMVECs and HAECs were isolated, electroblotted, and incubated with the following primary and secondary antibodies: (1) goat polyclonal anti-COX-2 (cat. N° sc-1747, dilution 1:500, Santa Cruz Biotechnologies, Santa Cruz, CA USA), secondary antibody mouse anti-goat IgG-HRP (cat. N° sc-2354, dilution 1:5000, Santa Cruz); (2) mouse monoclonal anti-AQP1 (cat. N° sc-55466, dilution 1:600, Santa Cruz), secondary antibody goat anti-mouse IgG-HRP (cat. N° sc-2005, dilution 1:5000, Santa Cruz); (3) mouse monoclonal anti-β-actin (cat. N° A5441, dilution 1:5000, Sigma, St. Louis, MO, USA), secondary antibody goat anti-mouse IgG-HRP (cat. N° sc-2005, dilution 1:5000, Santa Cruz); (4) rabbit polyclonal anti-TonEBP (cat. N° sc-13035, dilution 1:500, Santa Cruz), secondary antibody goat anti-rabbit IgG-HRP (cat. N° sc-12304, dilution 1:10000, Santa Cruz), as previously described .
Transfection of AQP1 and tonicity enhancer binding protein (TonEBP)/nuclear factor of activated T cells (NFAT)5 siRNA
A pool of three different small interfering RNA (siRNA) oligonucleotides to each target (AQP1 and TonEBP/NFAT5), as well as scrambled control siRNA were incubated with cells (2 × 105/well) in transfection medium, as previously described . After 24 h, fresh medium was added with or without HG (30.5 or 50.5 mmol/L), or HM (5.5 mmol/L glucose + 25 or 45 mmol/L mannitol), incubated for an additional 24 h, then subjected to Western analysis of COX-2, AQP1, TonEBP/NFAT5 and β-actin.
Tube formation assays
Tube formation assays were performed as previously described . Before the assay, cells were incubated in low serum (2.5 %) endothelial basal medium (EBM, BD Biosciences) without endothelial growth factors, with concentrations of control glucose (5.5 mmol/L, control), high glucose (30.5 or 50.5 mmol/l), high mannitol (5.5 mmol/L glucose + 25 or 45 mmol/L mannitol) for 24 h, in the presence or absence of the selective cyclooxygenase(COX)-2 inhibitor NS-398 at 1–10 μg/mL. In the assay testing the effect of siRNA to aquaporin (AQP)1 or TonEBP, cells were pretreated with high glucose or high mannitol for 24 h. At the end of incubations, cells were gently detached with 0.25 % trypsin–EDTA; trypsinized cells were then collected, counted and plated on Matrigel (at a density of 2 × 105 cells/50 μL Matrigel) for a further 16 h, in the presence or absence of control glucose, high glucose, high mannitol, with or without NS-398, or siRNA to AQP1 or TonEBP.
Cell migration assay
Cell migration was measured using the CytoSelect™ cell migration assay (Cell Biolabs, San Diego, CA, USA), according to the manufacturer’s instructions. Following a 24 h starvation period in 2 % fetal calf serum (FCS)/endothelial cell growth medium (EGM), cells were resuspended at 4 × 105 cells/mL in EGM and then placed in a separate well of a 96-well feeder tray containing 150 μL of migration media (EGM with control glucose concentration (5.5 mmol/L, control), high glucose (HG 30.5 mmol/L) or high mannitol (HM HM, 5.5 mmol/L glucose + 25 mmol/L mannitol)). One hundred and fifty microliters of assay controls, consisting of EGM supplemented with 10 % FCS (positive control) and basal EGM (negative control), were also tested in triplicate.
Electrophoretic mobility gel shift assay
Nuclear proteins were extracted from treated or untreated endothelial cells and subjected to electrophoretic mobility gel shift assay, as previously described . Double-stranded synthetic oligonucleotides of the nuclear factor (NF)-κB motif (5′-AGT TGA GGG GAC TTT CCC AGG C-3′ and 5′-CCT GGG AAA GTC CCC TCA ACT-3′) or of the Tonicity enhancer element (5′-GGT TTC TCC ACC TTT TCC GCT G-3′) were labeled with [γ-32P]ATP.
Immunoblotting of TonEBP
15 µg of nuclear extracts used for EMSA and of cytosolic extracts were electroblotted and incubated with either a primary rabbit polyclonal anti-TonEBP (cat. N° sc-13035, dilution 1:500, Santa Cruz), secondary antibody goat anti-rabbit IgG-HRP (cat. N° sc-12304, dilution 1:10,000, Santa Cruz); or an anti-lamin B antibody (Santa Cruz), as previously described .
Preparation of transit TKO-siRNA complexes and intravitreal injections of non-viral siRNA
Non-viral siRNA delivery into the mouse retina in vivo was done using a modified version of published methods . For monitoring transfection efficacy we used scrambled siRNA conjugated with a Cy3 fluorochrome provided by Mirus (Mirus Bio, Madison, WI, USA). Accordingly, 1.33 μL (25 nM) of Cy3-conjugated scrambled siRNA or Cy3-conjugated AQP1-siRNA (Ambion) were combined with 0.5 μL of Transit-TKO (Mirus) in a final volume 10 μL sterile H2O, and incubated for 30 min at room temperature. Wild-type C57BL/6 mice and age-sex matched D2.B6-Ins2 Akita diabetic mice were anesthetized by intraperitoneal injection of ketanest/xylazine (ketanest, 100–125 mg/kg; xylazine, 10–12.5 mg/kg). Intravitreal injections of phosphate-buffered saline (PBS, sham group, N = 7 wild-type C57BL/6 mice and N = 7 D2.B6-Ins2 Akita mice), or scrambled-siRNA (N = 7 wild-type C57BL/6 mice and N = 7 D2.B6-Ins2 Akita mice), or AQP1-siRNA (N = 7 wild-type C57BL/6 mice and N = 7 D2.B6-Ins2 Akita mice) were performed under a dissecting microscope with a 32 gauge needle attached to a 5 μL glass syringe (Hamilton, Reno, NV, USA). The needle was positioned 1 mm posterior to the limbus, where 5 μL of the solution were slowly (in 3–5 s) injected into the vitreous chamber of the eye. Injections were repeated after 72 h and 1 week from the first injection.
Tissue preparation and histological evaluation of vessel density
After the induction of anesthesia, retinas from D2.B6-Ins2 Akita diabetic mice and age/sex-matched C57/BL6 control mice were removed, embedded in optimal-cutting-temperature (OCT) medium, frozen on dry ice, and stored at −70 °C until sectioning. For immunofluorescence staining, 5 μm thick sagittal and frontal cryosections were obtained by using a sliding cryotome. These sections were permeabilized, blocked for 30 min in PBS containing 1 % bovine serum albumin, and incubated for 1 h at 4 °C with purified primary antibody anti-CD31 or Cy3-conjugated anti-α-smooth muscle actin (ASMA). A non-immune IgG (Becton, Dickinson and Co., Franklin Lakes, New Jersey, USA) was used as the isotype control. After washing with PBS, retinal sections stained with anti-CD31 antibody were incubated with phycoerythrin (PE)-conjugated secondary antibody, washed, mounted, and viewed with an immunofluorescence microscope. Sections were counterstained with 4′, 6-diamidino-2-phenylindole (DAPI) to identify nuclei. For immunohistochemistry, retinas were embedded in five separate paraffin blocks. Paraffin-embedded limb sections were deparaffinized, rehydrated, and stained with a primary antibody against CD31. Sections were counterstained with hematoxylin and eosin for structural analysis and to identify nuclei. Arterioles and capillaries were counted in a blinded manner in five randomly selected fields at 10× magnification. Vascular images were captured by using an inverted light microscope (Olympus IX71), and analyzed by using the Image-J software (Media Cybernetics, Rockville, MD, USA). Vessel density was expressed as the number of arterioles or capillaries per mm2.
Two-group comparisons were performed by the Student’s t test for unpaired values. Comparisons of means of ≥3 groups were performed by analysis of variance (ANOVA), and the existence of individual differences, in case of significant F-values at ANOVA, tested by Scheffé’s multiple contrasts.
High glucose induces COX-2 expression in human endothelial cells through a hyperosmolar mechanism
AQP1 mediates high glucose-induced COX-2 expression in endothelial cells
High glucose promotes angiogenesis through hyperosmolarity-induced expression of COX-2 and its transcription factor TonEBP/NFAT5
The promoter region of the COX-2 gene also contains consensus sequences for NF-κB [33–36], and high glucose induces the expression of some genes also by activating NF-κB [33, 37]. In order to analyze the contribution of NF-κB to the hyperosmotic stress-induced expression of COX-2, we performed EMSA using NF-κB binding probe and nuclear extracts from osmotically stressed HAECs for 1–24 h. We found low, but detectable amounts of NF-κB DNA binding activities in unstimulated cells. After treatment with high glucose (1 and 3 h) and TNF-α (up to 24 h), but not with high mannitol or sodium chloride, we observed a time-dependent increase in NF-κB DNA-binding activity, suggesting that this transcription factor can cooperate to the expression of the COX-2 gene by high glucose, but not in response to high glucose-related hyperosmotic stress (Fig. 5b–c).
Retinas of D2.B6-Ins2 Akita diabetic mice exhibit high levels of hyperosmolarity-enhanced COX-2 expression and angiogenesis
Clinical consequences of type-1 diabetes result from the combination of a number of different factors, ranging from acidosis to metabolic changes, to biophysical derangements, such as hyperosmotic stress. Previous research has mostly focused on metabolic disorders induced by hyperglycemia and the underlying signaling pathways. Several lines of evidence presented here however indicate that a substantial contribution to the induction of vascular disease is given by the hyperosmolar stress related to hyperglycemia. We show here that concentrations of glucose attainable in diabetes induce COX-2 in human endothelial cells through an AQP1-dependent hyperosmolar mechanism and, through this mechanism, promote angiogenesis. Specifically, in diabetic Ins2Akita mice, retinal COX-2 and AQP1 are upregulated concomitant with increased angiogenesis, suggesting the relevance of our observations in an in vivo setting where hyperglycemia is the main driver of microvascular disease. Finally, hyperosmolarity, through an AQP1-dependent mechanism appears to be causally involved in angiogenesis in vivo, and interruption of the AQP1 axis mitigates in vivo increased angiogenesis in response to high glucose.
This report expands our previous findings that hyperosmotic stress induces endothelial ICAM-1 and VCAM-1 expression  by showing the involvement of COX-2-dependent pathological phenomena. The current findings provide evidence that hyperosmolarity is a biophysical mechanism through which excessive angiogenesis may occur in diabetes. Additionally, our findings detail part of the molecular signaling through which hyperosmolarity promotes such effects.
The involvement of AQP1 in hyperosmolarity-induced endothelial tubulization and angiogenesis [38–41] is of biological importance. AQP1 is a water channel protein widely expressed in vascular endothelial cells, which, when activated, increases cell membrane water permeability [42–44]. AQP1 protein is strongly expressed in human and animal models of highly proliferating microvessels  and the chick embryo chorioallantoic membrane . In human retinal epithelial cells, osmotic stress decreases AQP4 expression . Reduction in AQP1 expression by targeted siRNA inhibits hyperosmolarity-dependent angiogenesis. In general, angiogenesis requires endothelial cell proliferation, adhesion and migration. We found a significant decrease in network number and areas in AQP1-silenced cultures, indicating a lost capacity to organize tubuli in networks. This is in line with previous reports showing that AQP1 plays a key role in endothelial cell migration, an early fundamental step in angiogenesis [10, 46].
Data from the present study also provide a mechanistic explanation on how AQP1 is linked to endothelial cell migration and tubulization. We observed that high glucose, at levels of 30.5 mmol/L, corresponding to 450 mg/dL, a plasma level possibly found in uncontrolled diabetes—increases COX-2 expression. This effect is in part dependent on the hyperosmolar component of hyperglycemia, since mimicked by the exposure of cells to the metabolically inactive monosaccharides mannitol or l-glucose.
TonEBP/NFAT5, a rel/NF-κB family member, has been identified as a transcription factor that in response to hyperosmolarity activates the transcription of osmosensing genes, including aldose reductase and protein kinase C delta , TNF-α and monocyte chemoattractant protein (MCP)-1 [30, 34–36]. In renal medullary epithelial cells, hypertonic stress increased COX-2 promoter activity in a luciferase reporter assay [37, 48]. Also, hypertonic saline had been reported to induce COX-2 in rat macrophages  and HUVECs , but in experimental conditions that do not reproduce the diabetic milieu. The participation of NFAT transcription factors in the activation of COX-2 expression had also been already demonstrated in several cell types [31, 32, 51–54]. Indeed, previous research had shown that the angiogenic signaling involved in the induction of COX-2 by vascular endothelial growth factor (VEGF) in human endothelial cells requires the activation of NFAT proteins [51, 55]. Furthermore, TonEBP/NFAT5 is required for the hypertonic induction of COX-2 in renal epithelial cells . An upregulation of the NFAT-MMP-2 pathway had been also demonstrated in the development of metastatic osteosarcoma, where the secretion of active MMP-2 is under the transcriptional regulation of NFAT . Here however we provide the first evidence that the induction of COX-2 in endothelial cells is largely hyperosmolarity-related, and that TonEBP/NFAT5 is here involved, since (a) TonEBP/NFAT total abundance was increased in cells exposed to high glucose or high mannitol; (b) EMSA and Western analysis demonstrated a cytoplasm-to-nucleus redistribution of TonEBP/NFAT in endothelial cells; and (c) TonEBP/NFAT gene disruption prevented hyperosmolarity-related induction of COX-2. Of note, our data show that at least another signal transduction pathways activated by high glucose, but with lesser relevance to COX-2 expression and angiogenesis, such as the NF-κB pathway, is—conversely—not substantially induced by high mannitol, indicating a larger dependence of NF-κB activation on metabolic effects of glucose.
A number of studies have shown that hyperosmolarity (as tested by high mannitol) does not influence angiogenesis and/or COX-2 expression in endothelial cells [55, 56]. Culture conditions used in these studies may not reflect those used in our study. Our data show more robust effects when using glucose concentrations as high as 50.5 mM, or with lower concentrations but for prolonged times, which may more closely mimic diabetic pathophysiology. Concentrations of glucose outside the range tested here might exert different effects, therefore not completely ruling out the additional involvement of mechanisms different from hyperosmolarity. Nevertheless, our data clearly indicate that hyperosmolarity is an important part of the mechanisms through which chronic exposure to high glucose may promote angiogenesis and cardiovascular complications of diabetes.
We recognize some limitations of our study. Main ones are that (a) there is limited translability of murine data to humans; (b) molecular mechanisms by which TonEBP/NFAT operates on the COX-2 promoter are still incompletely understood; (c) we still need to close the circle of the in vivo causality demonstration involving the transcription factor TonEBP/NFAT5 as an additional osmosignaling effector by showing that the in vivo interruption of the TonEBP signaling mitigates the in vivo increased angiogenesis in response to high glucose. Such experiments are complicated by the lack of available transgenic mouse models of TonEBP knockouts. Such limitations might however be overcome in the future through the prolonged administration of drugs targeting TonEBP activation.
RM designed and performed the experiments, analyzed the data and wrote the manuscript; GG performed in vitro experiments and analyzed the data; PC performed in vitro experiments; FVR performed in vitro experiments; YJG conceived the experiments, provided advise and financial support, and corrected the final manuscript. RDC conceived, designed and interpreted the experiments, and corrected the final manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
This work was supported by grants from the Italian Ministry of University and Scientific Research (PRIN), the CARIPLO Foundation and Istituto Nazionale Ricerche Cardiovascolari (INRC), to RDC.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- UK Prospective Diabetes Study UKPDS) Group. Effect of intensive blood-glucose control with metformin on complications in overweight patients with type 2 diabetes (UKPDS 34. Lancet. 1998;352(9131):854–65.View ArticleGoogle Scholar
- Holman RR, Paul SK, Bethel MA, Matthews DR, Neil HA. 10-year follow-up of intensive glucose control in type 2 diabetes. N Engl J Med. 2008;359(15):1577–89.PubMedView ArticleGoogle Scholar
- Brownlee M. Biochemistry and molecular cell biology of diabetic complications. Nature. 2001;414(6865):813–20.PubMedView ArticleGoogle Scholar
- Paget C, Lecomte M, Ruggiero D, Wiernsperger N, Lagarde M. Modification of enzymatic antioxidants in retinal microvascular cells by glucose or advanced glycation end products. Free Radic Biol Med. 1998;25(1):121–9.PubMedView ArticleGoogle Scholar
- Basta G, Lazzerini G, Massaro M, Simoncini T, Tanganelli P, Fu C, Kislinger T, Stern DM, Schmidt AM, De Caterina R. Advanced glycation end products activate endothelium through signal-transduction receptor RAGE: a mechanism for amplification of inflammatory responses. Circulation. 2002;105(7):816–22.PubMedView ArticleGoogle Scholar
- Ishii H, Koya D, King GL. Protein kinase C activation and its role in the development of vascular complications in diabetes mellitus. J Mol Med. 1998;76(1):21–31.PubMedView ArticleGoogle Scholar
- Shanmugam N, Gaw Gonzalo IT, Natarajan R. Molecular mechanisms of high glucose-induced cyclooxygenase-2 expression in monocytes. Diabetes. 2004;53(3):795–802.PubMedView ArticleGoogle Scholar
- Madonna R, De Caterina R. Cellular and molecular mechanisms of vascular injury in diabetes–part I: pathways of vascular disease in diabetes. Vascul Pharmacol. 2011;54(3–6):68–74.PubMedView ArticleGoogle Scholar
- Zhang W, Liu H, Al-Shabrawey M, Caldwell RW, Caldwell RB. Inflammation and diabetic retinal microvascular complications. J Cardiovasc Dis Res. 2011;2(2):96–103.PubMedPubMed CentralView ArticleGoogle Scholar
- Moreno PR, Fuster V. New aspects in the pathogenesis of diabetic atherothrombosis. J Am Coll Cardiol. 2004;44(12):2293–300.PubMedView ArticleGoogle Scholar
- Madonna R, Montebello E, Lazzerini G, Zurro M, De Caterina R. NA +/H + exchanger 1- and aquaporin-1-dependent hyperosmolarity changes decrease nitric oxide production and induce VCAM-1 expression in endothelial cells exposed to high glucose. Int J Immunopathol Pharmacol. 2010;23(3):755–65.PubMedGoogle Scholar
- Dubois RN, Abramson SB, Crofford L, Gupta RA, Simon LS, Van De Putte LB, Lipsky PE. Cyclooxygenase in biology and disease. FASEB J. 1998;12(12):1063–73.PubMedGoogle Scholar
- Tsujii M, Kawano S, Tsuji S, Sawaoka H, Hori M, DuBois RN. Cyclooxygenase regulates angiogenesis induced by colon cancer cells. Cell. 1998;93(5):705–16.PubMedView ArticleGoogle Scholar
- Masferrer JL, Leahy KM, Koki AT, Zweifel BS, Settle SL, Woerner BM, Edwards DA, Flickinger AG, Moore RJ, Seibert K. Antiangiogenic and antitumor activities of cyclooxygenase-2 inhibitors. Cancer Res. 2000;60(5):1306–11.PubMedGoogle Scholar
- Amano H, Ito Y, Suzuki T, Kato S, Matsui Y, Ogawa F, Murata T, Sugimoto Y, Senior R, Kitasato H, et al. Roles of a prostaglandin E-type receptor, EP3, in upregulation of matrix metalloproteinase-9 and vascular endothelial growth factor during enhancement of tumor metastasis. Cancer Sci. 2009;100(12):2318–24.PubMedView ArticleGoogle Scholar
- Conway EM, Collen D, Carmeliet P. Molecular mechanisms of blood vessel growth. Cardiovasc Res. 2001;49(3):507–21.PubMedView ArticleGoogle Scholar
- Toomey DP, Murphy JF, Conlon KC. COX-2, VEGF and tumour angiogenesis. Surgeon. 2009;7(3):174–80.PubMedView ArticleGoogle Scholar
- Frank RN. Diabetic retinopathy. N Engl J Med. 2004;350(1):48–58.PubMedView ArticleGoogle Scholar
- Carmeliet P. Angiogenesis in health and disease. Nat Med. 2003;9(6):653–60.PubMedView ArticleGoogle Scholar
- Roy S, Kim D, Hernandez C, Simo R. Beneficial effects of fenofibric acid on overexpression of extracellular matrix components, COX-2, and impairment of endothelial permeability associated with diabetic retinopathy. Exp Eye Res. 2015;140:124–9.PubMedView ArticleGoogle Scholar
- Peeters SA, Engelen L, Buijs J, Chaturvedi N, Fuller JH, Schalkwijk CG, Stehouwer CD. Plasma levels of matrix metalloproteinase-2, -3, -10, and tissue inhibitor of metalloproteinase-1 are associated with vascular complications in patients with type 1 diabetes: the EURODIAB Prospective Complications Study. Cardiovasc Diabetol. 2015;14:31.PubMedPubMed CentralView ArticleGoogle Scholar
- Cosentino F, Eto M, De Paolis P, van der Loo B, Bachschmid M, Ullrich V, Kouroedov A, Delli Gatti C, Joch H, Volpe M, et al. High glucose causes upregulation of cyclooxygenase-2 and alters prostanoid profile in human endothelial cells: role of protein kinase C and reactive oxygen species. Circulation. 2003;107(7):1017–23.PubMedView ArticleGoogle Scholar
- Barber AJ, Antonetti DA, Kern TS, Reiter CE, Soans RS, Krady JK, Levison SW, Gardner TW, Bronson SK. The Ins2Akita mouse as a model of early retinal complications in diabetes. Invest Ophthalmol Vis Sci. 2005;46(6):2210–8.PubMedView ArticleGoogle Scholar
- Han Z, Guo J, Conley SM, Naash MI. Retinal angiogenesis in the Ins2(Akita) mouse model of diabetic retinopathy. Invest Ophthalmol Vis Sci. 2013;54(1):574–84.PubMedPubMed CentralView ArticleGoogle Scholar
- Madonna R, Di Napoli P, Massaro M, Grilli A, Felaco M, De Caterina A, Tang D, De Caterina R, Geng YJ. Simvastatin attenuates expression of cytokine-inducible nitric-oxide synthase in embryonic cardiac myoblasts. J Biol Chem. 2005;280(14):13503–11.PubMedView ArticleGoogle Scholar
- Madonna R, Geng YJ, Shelat H, Ferdinandy P, De Caterina R. High glucose-induced hyperosmolarity impacts proliferation, cytoskeleton remodeling and migration of human induced pluripotent stem cells via aquaporin-1. Biochim Biophys Acta. 2014;1842(11):2266–75.PubMedView ArticleGoogle Scholar
- Turchinovich A, Zoidl G, Dermietzel R. Non-viral siRNA delivery into the mouse retina in vivo. BMC Ophthalmol. 2010;10:25.PubMedPubMed CentralView ArticleGoogle Scholar
- Lang F, Busch GL, Ritter M, Volkl H, Waldegger S, Gulbins E, Haussinger D. Functional significance of cell volume regulatory mechanisms. Physiol Rev. 1998;78(1):247–306.PubMedGoogle Scholar
- Gately S, Li WW. Multiple roles of COX-2 in tumor angiogenesis: a target for antiangiogenic therapy. Semin Oncol. 2004;31(2 Suppl 7):2–11.PubMedView ArticleGoogle Scholar
- Esensten JH, Tsytsykova AV, Lopez-Rodriguez C, Ligeiro FA, Rao A, Goldfeld AE. NFAT5 binds to the TNF promoter distinctly from NFATp, c, 3 and 4, and activates TNF transcription during hypertonic stress alone. Nucleic Acids Res. 2005;33(12):3845–54.PubMedPubMed CentralView ArticleGoogle Scholar
- Favale NO, Casali CI, Lepera LG, Pescio LG, Fernandez-Tome MC. Hypertonic induction of COX2 expression requires TonEBP/NFAT5 in renal epithelial cells. Biochem Biophys Res Commun. 2009;381(3):301–5.PubMedView ArticleGoogle Scholar
- Velupillai P, Sung CK, Tian Y, Dahl J, Carroll J, Bronson R, Benjamin T. Polyoma virus-induced osteosarcomas in inbred strains of mice: host determinants of metastasis. PLoS Pathog. 2010;6(1):e1000733.PubMedPubMed CentralView ArticleGoogle Scholar
- Chen G, Shen X, Yao J, Chen F, Lin X, Qiao Y, You T, Lin F, Fang X, Zou X, et al. Ablation of NF-kappaB expression by small interference RNA prevents the dysfunction of human umbilical vein endothelial cells induced by high glucose. Endocrine. 2009;35(1):63–74.PubMedView ArticleGoogle Scholar
- Miyakawa H, Woo SK, Chen CP, Dahl SC, Handler JS, Kwon HM. Cis- and trans-acting factors regulating transcription of the BGT1 gene in response to hypertonicity. Am J Physiol. 1998;274(4 Pt 2):F753–61.PubMedGoogle Scholar
- Takenaka M, Preston AS, Kwon HM, Handler JS. The tonicity-sensitive element that mediates increased transcription of the betaine transporter gene in response to hypertonic stress. J Biol Chem. 1994;269(47):29379–81.PubMedGoogle Scholar
- Kojima R, Taniguchi H, Tsuzuki A, Nakamura K, Sakakura Y, Ito M. Hypertonicity-induced expression of monocyte chemoattractant protein-1 through a novel cis-acting element and MAPK signaling pathways. J Immunol. 2010;184(9):5253–62.PubMedView ArticleGoogle Scholar
- Zhao H, Tian W, Tai C, Cohen DM. Hypertonic induction of COX-2 expression in renal medullary epithelial cells requires transactivation of the EGFR. Am J Physiol Renal Physiol. 2003;285(2):F281–8.PubMedView ArticleGoogle Scholar
- Kaneko K, Yagui K, Tanaka A, Yoshihara K, Ishikawa K, Takahashi K, Bujo H, Sakurai K, Saito Y. Aquaporin 1 is required for hypoxia-inducible angiogenesis in human retinal vascular endothelial cells. Microvasc Res. 2008;75(3):297–301.PubMedView ArticleGoogle Scholar
- Saadoun S, Papadopoulos MC, Hara-Chikuma M, Verkman AS. Impairment of angiogenesis and cell migration by targeted aquaporin-1 gene disruption. Nature. 2005;434(7034):786–92.PubMedView ArticleGoogle Scholar
- Maruyama T, Kadowaki H, Okamoto N, Nagai A, Naguro I, Matsuzawa A, Shibuya H, Tanaka K, Murata S, Takeda K, et al. CHIP-dependent termination of MEKK2 regulates temporal ERK activation required for proper hyperosmotic response. EMBO J. 2010;29(15):2501–14.PubMedPubMed CentralView ArticleGoogle Scholar
- Umenishi F, Schrier RW. Hypertonicity-induced aquaporin-1 (AQP1) expression is mediated by the activation of MAPK pathways and hypertonicity-responsive element in the AQP1 gene. J Biol Chem. 2003;278(18):15765–70.PubMedView ArticleGoogle Scholar
- Carter EP, Olveczky BP, Matthay MA, Verkman AS. High microvascular endothelial water permeability in mouse lung measured by a pleural surface fluorescence method. Biophys J. 1998;74(4):2121–8.PubMedPubMed CentralView ArticleGoogle Scholar
- Saadoun S, Papadopoulos MC, Davies DC, Bell BA, Krishna S. Increased aquaporin 1 water channel expression in human brain tumours. Br J Cancer. 2002;87(6):621–3.PubMedPubMed CentralView ArticleGoogle Scholar
- Ribatti D, Frigeri A, Nico B, Nicchia GP, De Giorgis M, Roncali L, Svelto M. Aquaporin-1 expression in the chick embryo chorioallantoic membrane. Anat Rec. 2002;268(2):85–9.PubMedView ArticleGoogle Scholar
- Willermain F, Janssens S, Arsenijevic T, Piens I, Bolaky N, Caspers L, Perret J, Delporte C. Osmotic stress decreases aquaporin-4 expression in the human retinal pigment epithelial cell line, ARPE-19. Int J Mol Med. 2014;34(2):533–8.PubMedGoogle Scholar
- Clapp C, de la Escalera GM. Aquaporin-1: a novel promoter of tumor angiogenesis. Trends Endocrinol Metab. 2006;17(1):1–2.PubMedView ArticleGoogle Scholar
- Park J, Kim H, Park SY, Lim SW, Kim YS, Lee DH, Roh GS, Kim HJ, Kang SS, Cho GJ, et al. Tonicity-responsive enhancer binding protein regulates the expression of aldose reductase and protein kinase C delta in a mouse model of diabetic retinopathy. Exp Eye Res. 2014;122:13–9.PubMedView ArticleGoogle Scholar
- Pucci ML, Endo S, Nomura T, Lu R, Khine C, Chan BS, Bao Y, Schuster VL. Coordinate control of prostaglandin E2 synthesis and uptake by hyperosmolarity in renal medullary interstitial cells. Am J Physiol Renal Physiol. 2006;290(3):F641–9.PubMedView ArticleGoogle Scholar
- Zhang W, Zitron E, Homme M, Kihm L, Morath C, Scherer D, Hegge S, Thomas D, Schmitt CP, Zeier M, et al. Aquaporin-1 channel function is positively regulated by protein kinase C. J Biol Chem. 2007;282(29):20933–40.PubMedView ArticleGoogle Scholar
- Arbabi S, Rosengart MR, Garcia I, Maier RV. Hypertonic saline solution induces prostacyclin production by increasing cyclooxygenase-2 expression. Surgery. 2000;128(2):198–205.PubMedView ArticleGoogle Scholar
- Hernandez GL, Volpert OV, Iniguez MA, Lorenzo E, Martinez-Martinez S, Grau R, Fresno M, Redondo JM. Selective inhibition of vascular endothelial growth factor-mediated angiogenesis by cyclosporin A: roles of the nuclear factor of activated T cells and cyclooxygenase 2. J Exp Med. 2001;193(5):607–20.PubMedPubMed CentralView ArticleGoogle Scholar
- Duque J, Fresno M, Iniguez MA. Expression and function of the nuclear factor of activated T cells in colon carcinoma cells: involvement in the regulation of cyclooxygenase-2. J Biol Chem. 2005;280(10):8686–93.PubMedView ArticleGoogle Scholar
- Yiu GK, Toker A. NFAT induces breast cancer cell invasion by promoting the induction of cyclooxygenase-2. J Biol Chem. 2006;281(18):12210–7.PubMedView ArticleGoogle Scholar
- Yan Y, Li J, Ouyang W, Ma Q, Hu Y, Zhang D, Ding J, Qu Q, Subbaramaiah K, Huang C. NFAT3 is specifically required for TNF-alpha-induced cyclooxygenase-2 (COX-2) expression and transformation of Cl41 cells. J Cell Sci. 2006;119(Pt 14):2985–94.PubMedView ArticleGoogle Scholar
- Giurdanella G, Anfuso CD, Olivieri M, Lupo G, Caporarello N, Eandi CM, Drago F, Bucolo C, Salomone S. Aflibercept, bevacizumab and ranibizumab prevent glucose-induced damage in human retinal pericytes in vitro, through a PLA2/COX-2/VEGF-A pathway. Biochem Pharmacol. 2015;96(3):278–87.PubMedView ArticleGoogle Scholar
- Lupo G, Motta C, Giurdanella G, Anfuso CD, Alberghina M, Drago F, Salomone S, Bucolo C. Role of phospholipases A2 in diabetic retinopathy: in vitro and in vivo studies. Biochem Pharmacol. 2013;86(11):1603–13.PubMedView ArticleGoogle Scholar