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Open Access

Peer-reviewed

Research Article

Oxidized LDL, homocysteine, homocysteine thiolactone and advanced glycation end products act as pro-oxidant metabolites inducing cytokine release, macrophage infiltration and pro-angiogenic effect in ARPE-19 cells

  • Kannadasan AnandBabu,

    Roles Data curation, Formal analysis, Methodology, Software, Validation, Visualization, Writing – original draft

    Affiliations R.S. Mehta Jain Department of Biochemistry and Cell Biology, KBIRVO, Vision Research Foundation, Sankara Nethralaya, Chennai, India, School of Chemical and Biotechnology, SASTRA University, Thanjavur, India

    ⨯
  • Parveen Sen,

    Roles Data curation, Investigation, Resources

    Affiliation Shri Bhagwan Mahavir Vitreoretinal Services, Sankara Nethralaya, Chennai, India

    ⨯
  • Narayanasamy Angayarkanni

    Roles Conceptualization, Formal analysis, Funding acquisition, Methodology, Project administration, Resources, Supervision, Validation, Visualization, Writing – original draft, Writing – review & editing

    drak@snmail.org, angayar07@gmail.com

    Affiliation R.S. Mehta Jain Department of Biochemistry and Cell Biology, KBIRVO, Vision Research Foundation, Sankara Nethralaya, Chennai, India

    ⨯

Abstract

Age-related Macular Degeneration (AMD) is one of the major vision-threatening diseases of the eye. Oxidative stress is one of the key factors in the onset and progression of AMD. In this study, metabolites associated with AMD pathology more so at the systemic level namely, oxidized LDL (oxLDL), homocysteine (Hcy), homocysteine thiolactone (HCTL), advanced glycation end product (AGE) were evaluated for their pro-oxidant nature in a localized ocular environment based on in vitro studies in human retinal pigment epithelial cells (ARPE-19 cells). Human ARPE-19 cells were treated with pro-oxidants 50 μg/mL oxLDL, 500 μM Hcy, 500 nM HCTL, 100 μg/mL AGE, 200 μM H2O2 and 200 μM H2O2 with and without pre-treatment of 5 mM N-acetyl cysteine (NAC). The cytokines IL-6, IL-8 and vascular endothelial growth factor (VEGF) secreted from ARPE-19 cells exposed to pro-oxidants were estimated by ELISA. In vitro angiogenesis assay was performed with conditioned media of the pro-oxidant treated ARPE-19 cells in Geltrex-Matrigel coated 96-well plate. The human acute monocytic leukemia cell line (THP-1) was differentiated into macrophages and its migration in response to conditioned media of ARPE-19 cells insulted with the pro-oxidants was studied by transwell migration assay. Western blot was performed to detect the protein expression of Bax, Bcl-2 and NF-κB to assess apoptotic changes. The compounds involved in the study showed a significant increase in reactive oxygen species (ROS) generation in ARPE-19 cells (oxLDL; Hcy; AGE: p < 0.001 and HCTL: p < 0.05). NAC pre-treatment significantly lowered the oxidative stress brought about by pro-oxidants as seen by lowered ROS and MDA levels in the cells. Treatment with pro-oxidants significantly increased the secretion of IL-6 (oxLDL: p < 0.05; Hcy, HCTL and AGE: p < 0.01) and IL-8 cytokines (oxLDL: p < 0.05; HCTL: p <. 001 and AGE: p < 0.01) in ARPE-19 cells. Serum samples of AMD patients (n = 23) revealed significantly higher IL-6 and IL-8 levels compared to control subjects (n = 23) (IL6: p < 0.01 and IL8: p < 0.05). The pro-oxidants also promoted VEGF secretion by ARPE-19 cells compared to untreated control (oxLDL: p < 0.001; Hcy: p < 0.01; HCTL and AGE: p < 0.05). In vitro angiogenesis assay showed that the conditioned media significantly increased the tube formation in RF/6A endothelial cells. Transwell migration assay revealed significant infiltration of macrophages in response to pro-oxidants. We further demonstrated that the pro-oxidants increased the Bax/Bcl-2 ratio and increased the NF-κB activation resulting in pro-apoptotic changes in ARPE-19 cells. Thus, oxLDL, Hcy, HCTL and AGE act as pro-oxidant metabolites in RPE that promote AMD through oxidative stress, inflammation, chemotaxis and neovascularization.

Citation: AnandBabu K, Sen P, Angayarkanni N (2019) Oxidized LDL, homocysteine, homocysteine thiolactone and advanced glycation end products act as pro-oxidant metabolites inducing cytokine release, macrophage infiltration and pro-angiogenic effect in ARPE-19 cells. PLoS ONE 14(5): e0216899. https://doi.org/10.1371/journal.pone.0216899

Editor: Alfred S. Lewin, University of Florida, UNITED STATES

Received: February 6, 2019; Accepted: April 30, 2019; Published: May 14, 2019

Copyright: © 2019 AnandBabu et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.

Data Availability: All relevant data are within the manuscript and its Supporting Information files.

Funding: Financial support from Indian Council of Medical Research (ICMR), Govt. of India (Grant Number: BMS/FW/BIOCHEM/2015-21610/JUN-2015/15/TN/PVT) and Dept. of Biotechnology, Govt. of India (Grant number: BT/PR13630/BRB/10/776/2010) is acknowledged. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

Competing interests: The authors have declared that no competing interests exist.

Introduction

Age-related macular degeneration (AMD) is a multifactorial disease, characterized by degeneration of retinal pigment epithelium (RPE) and photoreceptors in the macula. It is the leading cause of blindness in the elderly in many developed countries [1]. The retina and RPE are highly exposed to oxidative stress conditions due to intense light, increased lipofuscin formation as well as hypoxia, all of which contribute to the generation of reactive oxygen species (ROS) thereby promoting AMD pathogenesis in the early stage of the disease [2]. Oxidative stress, deranged lipid metabolism and inflammation play a major role in the pathogenesis of AMD [3–5].

Oxidation of LDL is a key atherogenic phenomenon in cardiovascular diseases (CVD) [6]. There are shared risk factors and pathogenic mechanisms in AMD and CVD, though the association between the two has not been clearly established [7]. This study explored these pro-oxidant factors associated with LDL modification in the context of RPE dysfunction relevant to AMD.

Elevated concentrations of plasma oxidized low-density lipoprotein (oxLDL) is one of the risk factors for AMD [8]. Our previous study reported on the elevated serum oxLDL in AMD [9]. OxLDL is a known atherogenic metabolite that is pro-inflammatory in nature [10]. However, there are limited studies on the role of oxLDL in AMD pathology not only at the systemic level but also at the level of RPE in the eye. Picard et al reported on the sub-RPE accumulation of oxLDL along with basement membrane thickening associated with AMD pathology [11].

Several metabolites are associated with LDL oxidation. Elevated plasma homocysteine (Hcy) as well as homocysteine thiolactone (HCTL), are metabolites associated with the AMD pathology [12–14] as excess homocysteine affects the RPE structure and function [15]. Hcy brings about LDL oxidation through modification of LDL apoB [16].

The advanced glycation end product (AGE), a key pathophysiological metabolite is associated with cardiovascular diseases [17,18], stroke [19] and AMD [20]. The AGE levels associated with aging contributes to RPE dysfunction in the pathogenesis of choroidal neovascularization (CNV) in AMD [21–23]. AGE can also form modified LDL [24].

The aim of the study is to see if the pathogenic molecules associated with AMD namely oxLDL, Hcy, HCTL and AGE cause pro-oxidant, pro-inflammatory and pro-angiogenic responses in the local environment of RPE as evaluated in ARPE-19 cells in vitro.

Materials and methods

ARPE-19 culture

The human Retinal Pigment Epithelial cells, ARPE-19 (ATCC-CRL-2302) was cultured using Dulbecco’s Modified Eagle medium/Ham’s F12 medium (DMEM/F-12; Sigma-Aldrich, USA) supplemented with 10% Fetal Bovine Serum (FBS; Gibco, USA), Antibiotic-Antimycotic solution (Gibco, USA). At 80% confluency, they were used for the experiments in DMEM/F-12 supplemented with 1% FBS (low serum media). The cells were then exposed to 50 μg/mL oxLDL, 50 μg/mL Native LDL (N.LDL), 500 μM Hcy (Sigma-Aldrich, USA), 500 nM HCTL (Sigma-Aldrich, USA), 100 μg/mL AGE, 200 μM H2O2 (Merck, USA) and pre-treatment with 5 mM N-acetylcysteine (NAC; Sigma-Aldrich, USA).

THP-1 Macrophage culture

The human acute monocytic leukemia cell line, THP-1 (Riken, Japan) was differentiated into macrophages using 50 ng/mL phorbol 12-myristate-13-acetate (PMA; Sigma-Aldrich, USA) for 48 h with Roswell Park Memorial Institute 1640 medium (RPMI 1640; Biowest, France), supplemented with 10% FBS. After 48 h, they were subjected to the experimental conditions.

LDL isolation by density gradient method

LDL was isolated from human plasma by density gradient method using Optiprep (60% Iodixanol solution) (Axis-Shield, Norway) by the method of Davies et al [25]. Human plasma was mixed with Optiprep to obtain 12% iodixanol as a working solution. Optiprep was mixed with PBS to arrive at 9% Iodixanol solution which was dispensed into Optiseal centrifuge tubes (Beckman Coulter, USA) and 3 mL of the iodixanol working solution was carefully under-layered with a syringe and metal cannula. The tubes were placed in NVT 65 near-vertical rotor (Beckman Coulter, USA) and centrifuged at 60,000 rpm for 3 h at 16°C in a Beckman Optima XL-100 ultracentrifuge (Beckman Coulter, USA). LDL separated as interphase was aspirated with syringe and metal cannula and concentrated using SpeedVac Concentrator (Thermo Fisher Scientific, USA).

In vitro oxidation of LDL and validation of LDL oxidation

The oxLDL was generated by incubating the plasma LDL with 10 μM CuCl2 at 37°C for 24 h [26]. Oxidation of LDL was confirmed based on the shift in absorbance at 234 nm [27]. The A234 before and after oxidation was 0.3802 and 0.5442, respectively. In addition, peroxidation of LDL was measured by the determination of thiobarbituric acid-reactive substances (TBARS) and expressed as malondialdehyde (MDA) equivalents [28]. Native LDL (N.LDL) and the corresponding oxLDL showed MDA levels of 3.76 ± 1.86 and 65.97 ± 6.26, respectively showing oxidation of LDL. Reactive free amino groups in N.LDL and oxLDL were estimated using spectrophotometer (Beckman Coulter, USA) by the method of Urs P. Steinbrecher [29]. Accordingly, there was a 30% decrease in the reactive amino group in oxLDL compared to N.LDL indicating LDL oxidation.

Measurement of intracellular reactive oxygen species

ARPE-19 cells were plated in a 96-well plate at a density of 1 x 104 cells/well. The cells were washed with PBS and 10 μM 2’-7” dichlorofluorescein diacetate (DCFH-DA) (Sigma-Aldrich, USA) in serum-free media was added to each well and incubated for 30 min at 37°C. Excess unused DCFH-DA was removed, washed once with PBS followed by incubation with the compounds of interest and the fluorescence was measured using SpectraMax M2e (Molecular Devices, USA) at Ex485 nm and Em530 nm in kinetic mode for one hour. ROS production was expressed as relative fluorescence. NAC (5 mM) was used as antioxidant, while H2O2 (200 μM) was used as the pro-oxidant (positive control). The cell homogenates were used in the MDA assay according to the method of Yokode et al., [28] to assess the intracellular oxidative stress.

MTT assay for cell viability

Cells were plated in a 96-well plate at a density of 1 x 104 cells/well. After exposing the cells to the compound of interest for 3 h, 24 h, 48 h and 72 h, media were aspirated and 0.5 mg/mL MTT (3-(4, 5-dimethylthiazolyl-2)-2, 5-diphenyltetrazolium bromide) (Molecular Probes, USA) was added and incubated for 4 h at 37°C. The formazan crystals formed were dissolved in dimethyl sulfoxide (DMSO) and the absorbance was measured at 570 nm and 650 nm as reference wavelengths using SpectraMax M2e. Cell viability was expressed as relative percentage to the untreated control.

Gene expressions by Real-Time PCR

RNA was isolated from the treated cells using TRI reagent (Favorgen Biotech Corp, Taiwan) and the cDNA conversion was performed using iScript cDNA synthesis (Biorad, Hercules, USA). The cDNA was used to determine the VEGF, α-SMA and NFE2L2 (Nrf2) gene expressions by Real-Time Polymerase Chain Reaction (qPCR), which was performed with the CFX96 Touch Real-Time detection system (Bio-Rad, USA) using SYBR Green chemistry (Roche, Germany). The qPCR conditions were 95°C for 10 min, followed by 40 cycles of 95°C for 15 s, 60°C for 15 s and 72°C for 20 s. The primer sequences are as given in the supplementary data (S1 Table). The comparative 2(-ΔΔCt) method was used to analyze the results of the genes of interest relative to the internal control gene (18S rRNA) [30] and expressed as fold change after normalizing to the untreated control.

Protein expression by western blotting

The cell lysate was prepared with RIPA (Radioimmunoprecipitation assay) buffer and the total protein estimation was measured using Pierce BCA protein assay kit (Thermo Fisher Scientific, USA) as per the manufacturer’s instructions. The protein resolved in 10% SDS-PAGE was transferred onto Hybond-P PVDF membrane (Amersham Pharmacia Biotech, UK), blocked with 5% BSA (Company, country) and probed with primary antibodies for pNF-κB, NF-κB (Cell Signaling Technology, USA), Bcl-2 (Thermo Fisher Scientific, USA), Bax and β-actin (Santa Cruz Biotechnology, USA). Then the blots were probed with corresponding species-specific HRP-conjugated secondary antibodies (Santa Cruz Biotechnology, Santa Cruz, CA, USA) and developed with Amersham ECL Prime Western Blotting Detection Reagent (GE Healthcare, UK) and the images were captured using FluorChem FC3 gel documentation system (Protein Simple, California, USA). The intensity of the bands were assessed using Image-J software (NIH, Bethesda, USA). β-actin was used as loading control.

Cytokine estimation

As per the published method of Holtkamp et al, the transwell filters (Costar; 12mm diameter, 0.4 μm pore size) coated with 160 μL of 1:40 dilution of Geltrex-Matrigel (Thermo Fisher Scientific, USA) in DMEM/F-12 medium and air-dried overnight. ARPE-19 cells (1 x 105) were cultured on transwell inserts in low serum media (200 μL per transwell) while the lower compartment had 1.0 mL medium and grown for 19 days. Trans-epithelial electrical resistance (TEER) was measured using EVOM2 Epithelial Voltohmmeter (World Precision Instruments, USA) to ensure RPE cell polarity. After subtracting the reading of transwell without cells, the resistance measured in Ω/cm2 were > 20 in all the wells indicative of RPE polarity [31]. The polarized nature of the cell was also evaluated based on increase in VEGF elaboration in transwells than cells grown in plates. The cells in transwell were then exposed to the pro-oxidant insults for 24 h. The basal conditioned media was then collected to measure IL-6 and IL-8 secretion by enzyme-linked immunosorbent assay (ELISA) (Peprotech, USA). In another set of experiment cells in transwell exposed to the pro-oxidant insults in the study for 24 h were evaluated for alpha-smooth muscle actin (α-SMA) gene expression as fibroblast marker, to check if transwell grown cells retain epithelial morphology to relate to the cytokine expression and this was compared cells grown in plates and exposed to similar insults using transforming growth factor-beta 1 (TGF-β1) as positive control.

Chemotactic assay

The ARPE-19 cells (3 x 104) were seeded to 24-well culture plate and allowed to grow till 80% confluency. The THP-1 Macrophage cells (2.5 x 105) was differentiated in transwell inserts of 8 μm pore size (Genetix Biotech Asia, India) separately. ARPE-19 cells were exposed to pro-oxidant insults for 24 h. The Chemotactic assay was performed after 24 h exposure by keeping the transwell inserts with THP-1 Macrophage over the ARPE-19 cells in the 24-well plates containing the conditioned media for 4 h. After 4 h, the THP-1 Macrophage was fixed with 4% paraformaldehyde (Merck, USA) and permeabilized with methanol (Sisco Research Laboratories Pvt. Ltd., India) and stained with Giemsa (Merck, USA). Non-migrated cells were scraped off from the upper surface and migrated cells in the lower surface of the inserts were observed under the bright field in Nikon Eclipse Ts2 microscope (Nikon Instruments Inc., USA) based on the stain at 10X magnification. Five random fields were captured for each insert and the number of migrated cells was counted. Three independent experiments were performed and the data are expressed as relative percentage to control.

In vitro angiogenesis assay

Tube formation assay was performed to check the secretion of pro-angiogenic factors from ARPE-19 using Geltrex-Matrigel. Initially, the 96-well plate was coated with Geltrex-Matrigel (35 μL/well) carefully without air bubbles and allowed to polymerize for 30 min at 37°C. Rhesus monkey Choroidal-retinal endothelial cells (RF/6A, #CRL1780, American Tissue Culture Collection) was subjected to low serum media for overnight and added at a density of 1.5 x 104 cells/well and mixed with 100 μL conditioned media of ARPE-19 treated with pro-oxidant conditions into 96-well plate coated with Geltrex-Matrigel. Vascular endothelial growth factor (VEGF; 10 ng/mL) was used as positive control. Tube formation on the gel surface was documented with Axio Observer Z.1 microscope (Carl Zeiss, Germany) after 4 h. Three random fields were captured in each well and the tube length was measured using the ImageJ software [32].

AMD patient recruitment for assessing pro-inflammatory cytokines in serum

As part of a prospective study in 2010–2013 in a tertiary eye care centre in south India, 23 AMD patients (Mean age: 68.8 ± 2.1 years, M/F: 17/6) and 23 healthy control subjects (Mean age: 53.7 ± 1.8 years, M/F: 14/9) were recruited in this study. The study was conducted in adherence to the principles of the Helsinki declaration and approved by the Ethics Sub-Committee of Vision Research Foundation, Sankara Nethralaya (Study Code: 149-2009-P, dated 29.08.2009). A written informed consent was obtained from the study participants. Detailed ophthalmic and medical evaluation was done and subjects with history of Diabetes Mellitus (DM), renal dysfunction, hepatic disease, or inflammatory diseases and presence of retinal diseases other than AMD such as high myopia, retinal dystrophies, central serous retinopathy, vein occlusion, diabetic retinopathy, and uveitis or similar outer retinal diseases which has been present prior to the age of 50 years were excluded. AMD diagnosis was based on the Age-Related Eye Disease Study (AREDS) guidelines [33]. The laboratory investigations of biochemical tests done and the clinical data are given in the supplementary data (S2 Table and S1 File). Serum IL-6 and IL-8 levels were estimated in AMD patients and control subjects by ELISA.

Statistics

All data are expressed as Mean ± SEM of 3 independent experiments done not less than duplicates unless indicated. Statistical significance was assessed by Student’s t-test. p < 0.05 was considered statistically significant.

Results

ROS generation after exposure to oxLDL and Hcy

The oxidative capability of the metabolites was assessed by intracellular ROS and MDA levels in ARPE-19 cells. A significant increase in the ROS level was observed in the ARPE-19 cells exposed to oxLDL compared to untreated and N.LDL treated cells (p < 0.001). Hcy, AGE (p < 0.001) and HCTL (p < 0.05) also promoted ROS generation and thus acted as significant pro-oxidants. The anti-oxidant, NAC significantly reduced the ROS levels induced by the metabolites (Fig 1A). The intracellular MDA was significantly increased by the metabolites studied. This was lowered by the NAC treatment, thus showing the oxidative stress in ARPE-19 cells caused by the metabolites (S1 Fig).

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Fig 1. ROS assay and pro-inflammatory cytokine levels.

(A) ROS assay in ARPE-19 cells by DCFH-DA method, (B) MTT assay for cell viability in ARPE-19 cells, (C) IL-8 and (D) IL-6 estimation in basal conditioned media of ARPE-19 cells exposed to pro-oxidants conditions for 24 h by ELISA, (E) Serum IL-8 levels and (F) Serum IL-6 levels. Values are expressed as Mean ± SEM. *;#p < 0.05, **,##p < 0.01, ***;###;δδδp < 0.001, considered as significant. *Control vs pro-oxidants, #pro-oxidants vs NAC, δoxLDL vs N.LDL.

https://doi.org/10.1371/journal.pone.0216899.g001

Cell viability assay

MTT assay was performed to find out the cytotoxic effect of the compounds studied in ARPE-19 cells. Cells were treated with 50 μg/mL oxLDL, 50 μg/mL N.LDL, 500 μM Hcy, 500 nM HCTL, 100 μg/mL AGE and 200 μM H2O2 for various time points. The cells were viable under all the treatment conditions and no significant cell death was observed at 24 h (Fig 1B). This was further substantiated by the trypan blue assay that showed less than 10% cell death with pro-oxidants treatment at both 24 h and 72 h, which was not statistically significant (S2 Fig). However, there was around 20 percent reduction in the MTT assay with the metabolites at 72 h, which can be attributed to the loss of mitochondrial activity (S3 Fig). Thus the metabolites caused no significant cell death in spite of their pro-oxidant effect in ARPE-19 cells.

Pro-inflammatory cytokines are secreted by APRE-19 cells on treatment with oxLDL, Hcy and AGE

Increased oxidative stress can trigger the inflammatory response in RPE. Therefore, IL-6 and IL-8 were evaluated amongst the cytokines reportedly associated with AMD. IL-8 secretion by ARPE-19 cells was significantly elevated on treatment with oxLDL (p < 0.05), AGE and H2O2 (p < 0.01). However, HCTL showed maximal induction (p < 0.001), while Hcy treatment did not alter it significantly (Fig 1C). IL-6 secretion by ARPE-19 cells was significantly elevated with oxLDL (p < 0.05) and AGE treatment (p < 0.01). Hcy and HCTL treatments showed maximal IL-6 release similar to that of H2O2 treatment (p < 0.01) (Fig 1D). Thus, the pro-oxidants studied promoted inflammatory response in ARPE-19 cells.

When these specific inflammatory markers were assessed at the systemic level, the serum IL-8 and IL-6 levels were found to be significantly elevated in the AMD patients (10.48 ± 1.79 pg/mL and 12.97 ± 1.46 pg/mL, respectively) compared to control subjects (6.07 ± 0.76 pg/mL and 8.76 ± 0.62 pg/mL, correspondingly) (Fig 1E and 1F). Thus, inflammation is observed at the systemic level in AMD as seen by the cytokine markers studied. S2 Table shows the systemic biochemical details of the AMD patients, wherein significantly altered plasma lipid profile was observed in terms of increased total cholesterol, triglycerides and very low-density lipoprotein (VLDL).

Cells grown in transwell inserts were evaluated for their epithelial nature. The gene expression of the fibroblastic marker, α-SMA was not increased in the cells treated with the pro-oxidants at the concentration and time point studied (S4 Fig). Hence, the cytokines measured in transwell are from the polarized and epithelial form of RPE cells. However, a significant increase in α-SMA was observed in cells cultured in tissue culture plates in response to all the pro-oxidants, similar to the insult of TGF-β1 at 5 ng/mL (positive control).

Increased VEGF secretion with oxLDL, Hcy and AGE treatment

Oxidative stress and chronic inflammation in the RPE and retina are reported to be associated with choroidal neovascularization in AMD. Hence, we measured the VEGF expression in ARPE-19 exposed to pro-oxidant metabolites. Treatment with oxLDL, Hcy, HCTL and AGE showed a significant increase in the VEGF mRNA and protein expression at 24 h (Fig 2A). The VEGF levels in vitreous of AMD patients (83.98 ± 20.31 pg/mL) was significantly higher compared to idiopathic Macular Hole subjects (30.15 ± 7.78 pg/mL) (Fig 2B). These results showed that these metabolites pave way for the wet AMD.

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Fig 2. Pro-angiogenic effect of the pro-oxidants in ARPE-19 cells.

(A) VEGF gene expression and protein secretion in ARPE-19 cells. (a) VEGF gene expression was quantified by qPCR in ARPE-19 cells exposed to pro-oxidant conditions for 24 h, (b) VEGF secretion was estimated by ELISA in conditioned media of ARPE-19 cells exposed to pro-oxidant conditions for 24 h. (B) Vitreous VEGF levels in Macular Hole and AMD. VEGF protein levels in vitreous of idiopathic Macular Hole subjects and AMD patients were estimated by ELISA. (C) In vitro Angiogenesis Assay. (a) RF/6A cells were treated with conditioned media of ARPE-19 exposed to pro-oxidant conditions and 10 ng/mL VEGF for 4 h and images were captured using Axio Observer Z.1 microscope at 5X magnification, (b) Bar graph represents the quantification of tube length measured using ImageJ software and expressed as relative percentage to control. The data are represented as Mean ± SEM. *;#p < 0.05, **;##p < 0.01, ***p < 0.001, considered as significant. *Control vs pro-oxidants, #H2O2 vs NAC.

https://doi.org/10.1371/journal.pone.0216899.g002

Angiogenesis is promoted by oxLDL, Hcy and AGE

As the VEGF secretion increased by ARPE-19 under oxidative stress, the effect of conditioned media of ARPE-19 cells exposed to the pro-oxidants was assessed for pro-angiogenic effect by in vitro angiogenesis assay in RF6A endothelial cells. There was a significant increase in tube formation on exposures to oxLDL, Hcy, HCTL, AGE and H2O2 by 67.7%, 36.9%, 56.2%, 41.9% and 67.2%, respectively compared to control. VEGF treatment used as a positive control showed an increase by 167.5% and NAC treatment decreased this by 15% (Fig 2C). This shows that oxLDL, Hcy, HCTL and AGE promote angiogenesis which is characteristic of wet AMD.

Oxidative stress promotes chemotaxis of macrophages

Macrophage infiltration is one of the key events in the pathogenesis for choroidal neovascularization in wet AMD. Hence, we performed the transwell migration assay to assess the macrophage infiltration in response to the secretion of ARPE-19 cells exposed to pro-oxidant conditions. This assay showed that there was a significant increase in the migration of macrophages in response to oxLDL, Hcy, AGE by 15.3%, 13.2% and 14.4%, respectively compared to control. NAC treatment showed an 11% decrease compared to H2O2-alone treatment (Fig 3A and 3B). This result indicates that the oxidative stress induced by these metabolites in ARPE-19 cells promote secretion of pro-inflammatory cytokines, which in turn causes macrophage infiltration.

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Fig 3. Chemotactic assay of THP-1 macrophages.

(A) Transwell migration of THP-1 macrophage in response to the cytokine secretion of ARPE-19 cells exposed to pro-oxidant conditions for 24 h was assessed after 4 h incubation. The migrated macrophages were stained with Giemsa stain and five random fields were captured per well with Nikon Eclipse Ts2 microscope at 10X magnification. (B) Bar chart showing the number of migrated macrophages, represented as relative percentage to control. Values are expressed as Mean ± SEM, n = 3. *p < 0.05, δδδp < 0.001, considered as significant. *Control vs pro-oxidants, #H2O2 vs NAC, δoxLDL vs N.LDL.

https://doi.org/10.1371/journal.pone.0216899.g003

Oxidative stress promotes pro-apoptotic changes via NF-κB signaling

To investigate whether the pro-oxidants induce pro-apoptotic changes in ARPE-19 cells, the protein expression of Bcl-2 (anti-apoptotic) and Bax (pro-apoptotic), as well as the activation of the pro-apoptotic transcription NF-κB protein by its phosphorylation were evaluated. There was a significant increase in the Bax/Bcl-2 ratio with the pro-oxidant treatments (Fig 4A and 4B) along with significant activation of NF-κB in ARPE-19 cells (Fig 4C and 4D). Further, NFE2L2, transcription factor which is known to be increased in oxidative stress as a defence was evaluated and found to be increased by the pro-oxidants treatment (Fig 4E). With HCTL, NFE2L2 expression was significantly lower though NF-κB was increased. However, net oxidative stress was observed in HCTL treament with respect to ROS and MDA levels. Interestingly, NAC treatment further increased the NFE2L2 expression in RPE unlike in other cells reported [34]. Annexin V staining supported the pro-apoptotic changes of ARPE-19 cells under the pro-oxidant conditions (S5 Fig).

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Fig 4. Pro-apoptotic changes in ARPE-19 cells.

(A) Bax and Bcl-2 protein expression in ARPE-19 under the pro-oxidants conditions treated for 24 h was assessed by western blot. (B) Densitogram analysis of Bax/Bcl-2 ratio normalized to control. (C) pNF-κB and NF-κB protein expression in ARPE-19 under the pro-oxidants conditions treated for 24 h was assessed by western blot. (D) Densitogram analysis of pNF-κB/NF-κB ratio normalized to control. (E) NFE2L2 gene expression was quantified by qPCR in ARPE-19 cells exposed to pro-oxidant conditions for 24 h. Values are expressed as Mean ± SEM, n = 3. *;#p < 0.05, **,##p < 0.01, ***p < 0.001, considered as significant. *Control vs pro-oxidants, #H2O2 vs NAC.

https://doi.org/10.1371/journal.pone.0216899.g004

Discussion

Oxidative stress is one of the major contributors to the pathogenesis of AMD. Many systemic pro-oxidant metabolites are formed during oxidative stress pathologies such as the lipid-derived reactive aldehydes, proteins / amino acid oxidative markers such as nitrotyrosine, nucleic acid oxidation product such as 8-hydroxy deoxyguanosine, the prostaglandin derived F2-isoprostanes and the redox imbalance marker, Hcy. Association of such metabolites with AMD pathology has been reported widely [13,35–38].

This study focussed on oxLDL which is not extensively studied in RPE in the context of AMD. In our previous study in AMD, we found that serum oxLDL was significantly elevated in AMD patients. The study showed that compared to native LDL, oxLDL increases ROS in ARPE-19 cells. The oxLDL level is reported as a biomarker of many oxidative stress involving pathologies such as atherosclerosis, cerebral infarction and AMD as well [39]. Formation of lipid-protein adducts such as MDA-lysine and 4-HNE-lysine on apolipoprotein B can induce ROS formation [40]. ROS generation as well as metabolism of oxLDL, can promote RPE cell dysfunction due to pathological stress response contributing to AMD pathology [41].

Though controversial, Hcy at the systemic level has been associated with AMD [42]. Our previous study showed that high plasma Hcy and HCTL levels were not significantly different from that of the age-matched controls [9]. However, recent studies reveal that it can potentially cause RPE dysfunction [15,43]. This study explored to delineate their effect localized to RPE. Accordingly, Hcy and HCTL increased the ROS levels in ARPE-19 cells acting as pro-oxidants. Hcy can undergo cyclization to form HCTL which brings about N-homocysteinylation of proteins including that of LDL. These Hcy-N-proteins are capable of initiating oxidative damages [44,45]. HCTL, released from homocysteinylated LDL causes oxidation of cholesterol [46]. Hcy and HCTL also mediate MDA accumulation in the microvascular endothelial cells as reported by us earlier [47]. More studies are warranted to delineate its role in AMD pathology at the local environment rather than relating to systemic hyperhomocysteinemia.

Accumulation of AGE with aging is associated with drusens and is known to promote receptor for AGE (RAGE) mediated neovascularization and apoptosis in AMD [23]. AGE levels increase with oxidative stress and the accumulated AGE, in turn, can increase ROS levels apart from glycating the proteins [48]. Methylglyoxal promotes cell death through ROS generation in ARPE-19 cells [49]. The study shows the comparison of the metabolites including that of the AGE treatment that can promote AMD pathology at the level of oxidative stress, inflammation, apoptosis and pro-angiogenic effect.

Increase in IL-6 and IL-8 secretions were observed in ARPE-19 cells on treatment with the pro-oxidants studied. Evidences based on histological studies has shown chronic inflammation in RPE and choroid with infiltration of lymphocytes and macrophages in AMD eyes [50]. Interestingly, serum pro-inflammatory cytokines, IL-6 and IL-8 were found to be high in AMD patients. Thus, there is a systemic inflammation as well as the inflammatory component of the RPE environment involved in AMD pathology. While a recent report states that no systemic changes in serum or aqueous humour in any of the cytokine was observed in AMD, a panel of altered cytokines has also been reported in AMD [51,52]. While the method of detection seems to be a point of concern, more studies in larger groups are warranted to understand the local versus systemic markers of the inflammation status in AMD.

Increased VEGF expression observed on pro-oxidant treatment in ARPE-19 reveals that the local environment of RPE is susceptible to oxidative stress. In vitro angiogenesis assay revealed factors secreted by RPE in response to the intracellular ROS generated promote neovascularization. There was a significant increase in VEGF levels in vitreous of AMD patients compared to idiopathic Macular Hole subjects. However, it is shown in a small sample size which is a limitation in the study. Inflammasome activation by lipids is reported both at the systemic level and in the RPE local environment in AMD [53]. Moreover, oxLDL, Hcy and AGE induce VEGF secretion also in macrophages [54–57]. The role of macrophages in the pathological neovascularization remains elusive. While Apte et al., 2006 showed macrophages are protective in limiting neovascular process as seen in laser-induced CNV mice model, earlier studies had shown that depletion of macrophages blocked neovascularization in mouse models [58,59]. However, CNV is associated with specific M2 polarized macrophages [60]. Monocyte/macrophage recruitment in response to cytokine secretion is reported in cell models [61]. We found THP-1 macrophage chemotaxis in response to cellular supernatant by the ARPE-19 exposed to pro-oxidants. Thus, the macrophage infiltration was mediated by cytokine elaborated by the ARPE-19 exposed to these pro-oxidant metabolites.

Oxidative stress induces pro-apoptotic changes in various cells [62–64]. The oxLDL induces apoptosis of RPE through activation of ERK-Bax/Bcl-2 signaling pathways [65]. We found that the pro-oxidants oxLDL, Hcy, HCTL and AGE increased the Bax to Bcl-2 ratio and activation of NF-κB, showing pro-apoptotic changes in ARPE-19. Activation of NF-κB inducing apoptosis in response to various stimuli such as oxLDL, Hcy and AGE has been reported earlier [64,66,67]. Interestingly, HCTL seems to be more deleterious as there is a significant decrease in NFE2L2 expression which is supported by the observation that IL-8 secretion is maximal in HCTL treatment. Lowering of NFE2L2 expression reportedly promotes inflammation [68]. NAC treatment in RPE unlike in other cells did not suppress NFE2L2 expression and in fact further increased the expression over that of H2O2 treatment. This is probably characteristic of RPE and needs further studies. Earlier we had reported that PON2, an antioxidant increased by H2O2 treatment was further increased with NAC treatment in ARPE-19 cells [69].

Oxidative stress induces epithelial to mesenchymal transition that leads to functional deficiencies of RPE in AMD [70]. In this study, only the cytokine release and chemotactic response were done in transwell grown polarized cells wherein the cells are epithelial in nature. However, the rest were done in plate culture where RPE exhibits mesenchymal change with the pro-oxidants which is a study limitation. There are both epithelial and mesenchymal RPE in AMD and more studies are required in the in vivo condition to evaluate EMT with disease progression.

Conclusion

The study showed that the metabolites studied induce intracellular ROS generation in ARPE-19 cells promoting secretion of pro-inflammatory cytokines. The cytokines recruit macrophages at the site of RPE and induce VEGF secretion promoting neovascularization. Moreover, these pro-oxidant metabolites induce pro-apoptotic changes in RPE through NF-κB signaling.

Supporting information

S1 Fig. MDA assay in ARPE-19 cells.

ARPE-19 cells were exposed to metabolites namely 50 μg/mL oxLDL, 500 μM Hcy, 500 nM HCTL, 100 μg/mL AGE, 200 μM H2O2 for 24 hours and with or without pre-treatment with 5 mM NAC for 1 hour. After exposure, the cells were lysed with 0.5% Triton X 100 and measured the MDA formed by MDA assay. The data are represented as Mean ± SEM. *;#p < 0.05, **,##p < 0.01, considered as significant. *Control vs pro-oxidants; #pro-oxidants vs NAC.

https://doi.org/10.1371/journal.pone.0216899.s001

(TIF)

S2 Fig. Trypan Blue assay for cell viability in ARPE-19 cells.

ARPE-19 cells were exposed to pro-oxidants for 24 h (A) and 72h (B). The cell viability was measured by Trypan Blue assay. At the end of the exposure, the cell suspension after trypsinization was mixed with 0.4% trypan blue solution (1:1) and counted the stained (dead) and unstained (viable) cells in a hemocytometer. The data are expressed as cell viability (%) relative to control and is a mean of three independent experiments (Mean ± SEM).

https://doi.org/10.1371/journal.pone.0216899.s002

(TIF)

S3 Fig. MTT assay in ARPE-19 cells.

MTT assay was performed at different time points such as 3, 24, 48, and 72 h with the exposures of 50 μg/mL oxLDL, 500 μM Hcy, 500 nM HCTL, 100 μg/mL AGE, 200 μM H2O2 and 5 mM NAC pre-treatment with 200 μM H2O2. Nearly 20% fall in the mitochondrial activity was observed with the metabolites treatment at 72 h with all the exposures except 100 μg/mL AGE (< 5%).

https://doi.org/10.1371/journal.pone.0216899.s003

(TIF)

S4 Fig. α-SMA gene expression in ARPE-19.

α-SMA gene expression was quantified by qPCR in ARPE-19 cells exposed to pro-oxidant conditions for 24 h. (A) ARPE-19 cells grown on 12-well transwell inserts, (B) ARPE-19 cells grown in 12-well tissue culture plate. The fold change (Y-axis) is calculated after normalizing to untreated control as detailed in the method section 2.7. The data are represented as Mean ± SEM. *p < 0.05, ***p < 0.001, considered as significant. *Control vs pro-oxidants.

https://doi.org/10.1371/journal.pone.0216899.s004

(TIF)

S5 Fig. Annexin V staining showing apoptotic changes in ARPE-19 cells.

ARPE-19 cells were exposed to pro-oxidants for 24 h and apoptotic changes were observed by Annexin V staining. FITC labelled Annexin V was indicated by green fluorescence. Image magnification, 40X.

https://doi.org/10.1371/journal.pone.0216899.s005

(TIF)

S1 Table. List of primers used for Real-Time PCR.

https://doi.org/10.1371/journal.pone.0216899.s006

(DOC)

S2 Table. Biochemical parameters in AMD and control.

Data are expressed as Mean ± SEM; M: Male; F: Female; HDL: High-density lipoprotein; LDL: Low-density lipoprotein; VLDL: Very low-density lipoprotein; TC: Total cholesterol. NS: Not significant.

https://doi.org/10.1371/journal.pone.0216899.s007

(DOC)

S1 File. Clinical data of participants recruited in the study.

https://doi.org/10.1371/journal.pone.0216899.s008

(XLS)

References

  1. 1. Lim LS, Mitchell P, Seddon JM, Holz FG, Wong TY. Age-related macular degeneration. Lancet. Elsevier Ltd; 2012;379: 1728–38.
  2. 2. Cai J, Nelson KC, Wu M, Sternberg P, Jones DP. Oxidative damage and protection of the RPE. Prog Retin Eye Res. 2000;19: 205–21. pmid:10674708
  3. 3. Xu Q, Cao S, Rajapakse S, Matsubara JA. Understanding AMD by analogy: Systematic review of lipid-related common pathogenic mechanisms in AMD, AD, AS and GN. Lipids Health Dis. Lipids in Health and Disease; 2018;17: 1–13.
  4. 4. Zarbin M a. Current Concepts in the Pathogenesis of Age-Related Macular Degeneration. Cell. 2004;122: 598–614.
  5. 5. Jarrett SG, Boulton ME. Consequences of oxidative stress in age-related macular degeneration. Mol Aspects Med. 2012;33: 399–417. pmid:22510306
  6. 6. BOULLIER A, BIRD DA, CHANG M-K, DENNIS EA, FRIEDMAN P, GILLOTTE-TAYLOR K, et al. Scavenger Receptors, Oxidized LDL, and Atherosclerosis. Ann N Y Acad Sci. 2006;947: 214–223.
  7. 7. Pennington KL, DeAngelis MM. Epidemiology of age-related macular degeneration (AMD): associations with cardiovascular disease phenotypes and lipid factors. Eye Vis. 2016;3: 34. pmid:28032115
  8. 8. Javadzadeh A, Ghorbanihaghjo A, Bahreini E, Rashtchizadeh N, Argani H, Alizadeh S. Plasma oxidized LDL and thiol-containing molecules in patients with exudative age-related macular degeneration. Mol Vis. 2010;16: 2578–84. pmid:21151596
  9. 9. AnandBabu K, Bharathidevi S, Sripriya S, Sen P, Jaya Prakash V, Bindu A, et al. Serum Paraoxonase activity in relation to lipid profile in Age-related Macular Degeneration patients. Exp Eye Res. 2016;152: 100–112. pmid:27693409
  10. 10. Lara-Guzmán OJ, Gil-Izquierdo Á, Medina S, Osorio E, Álvarez-Quintero R, Zuluaga N, et al. Oxidized LDL triggers changes in oxidative stress and inflammatory biomarkers in human macrophages. Redox Biol. Elsevier; 2018;15: 1–11. pmid:29195136
  11. 11. Picard E, Houssier M, Bujold K, Sapieha P, Lubell W, Dorfman A, et al. CD36 plays an important role in the clearance of oxLDL and associated age-dependent sub-retinal deposits. Aging (Albany NY). 2010;2: 981–9.
  12. 12. Coral K, Raman R, Rathi S, Rajesh M, Sulochana KN, Angayarkanni N, et al. Plasma homocysteine and total thiol content in patients with exudative age-related macular degeneration. Eye (Lond). 2006;20: 203–207. pmid:15803172
  13. 13. Huang P, Wang F, Sah BK, Jiang J, Ni Z, Wang J, et al. Homocysteine and the risk of age-related macular degeneration: a systematic review and meta-analysis. Sci Rep. Nature Publishing Group; 2015;5: 10585. pmid:26194346
  14. 14. Bharathselvi M, Biswas S, Raman R, Selvi R, Coral K, Narayanansamy A, et al. Homocysteine & its metabolite homocysteine-thiolactone & deficiency of copper in patients with age related macular degeneration—A pilot study. Indian J Med Res. 2016;143: 756–762. pmid:27748300
  15. 15. Ibrahim AS, Mander S, Hussein KA, Elsherbiny NM, Smith SB, Al-Shabrawey M, et al. Hyperhomocysteinemia disrupts retinal pigment epithelial structure and function with features of age-related macular degeneration. Oncotarget. Impact Journals, LLC; 2016;7: 8532–45. pmid:26885895
  16. 16. Vidal M, Sainte-Marie J, Philippot J, Bienvenue A. Thiolation of low-density lipoproteins and their interaction with L2C leukemic lymphocytes. Biochimie. 1986;68: 723–30. pmid:3089330
  17. 17. Peppa M, Uribarri J, Vlassara H. The role of advanced glycation end products in the development of atherosclerosis. Curr Diab Rep. 2004;4: 31–6. pmid:14764277
  18. 18. Falcone C, Bozzini S, D’Angelo A, Matrone B, Colonna A, Benzi A, et al. Plasma levels of soluble receptor for advanced glycation end products and coronary atherosclerosis: possible correlation with clinical presentation. Dis Markers. 2013;35: 135–40. pmid:24167358
  19. 19. Zimmerman GA, Meistrell M, Bloom O, Cockroft KM, Bianchi M, Risucci D, et al. Neurotoxicity of advanced glycation endproducts during focal stroke and neuroprotective effects of aminoguanidine. Proc Natl Acad Sci U S A. National Academy of Sciences; 1995;92: 3744–8.
  20. 20. Ishibashi T, Murata T, Hangai M, Nagai R, Horiuchi S, Lopez PF, et al. Advanced glycation end products in age-related macular degeneration. Arch Ophthalmol. 1998;116: 1629–32. pmid:9869793
  21. 21. Glenn JV, Mahaffy H, Wu K, Smith G, Nagai R, Simpson D a C, et al. Advanced glycation end product (AGE) accumulation on Bruch’s membrane: links to age-related RPE dysfunction. Invest Ophthalmol Vis Sci. 2009;50: 441–51. pmid:18676633
  22. 22. Chiu CJ, Taylor A. Dietary hyperglycemia, glycemic index and metabolic retinal diseases. Prog Retin Eye Res. Elsevier Ltd; 2011;30: 18–53. pmid:20868767
  23. 23. Glenn JV, Stitt AW. The role of advanced glycation end products in retinal ageing and disease. Biochim Biophys Acta. Elsevier B.V.; 2009;1790: 1109–16. pmid:19409449
  24. 24. Bucala R, Makita Z, Vega G, Grundy S, Koschinsky T, Cerami A, et al. Modification of low density lipoprotein by advanced glycation end products contributes to the dyslipidemia of diabetes and renal insufficiency. Proc Natl Acad Sci U S A. 1994;91: 9441–5. pmid:7937786
  25. 25. Davies IG, Graham JM, Griffin BA. Rapid separation of LDL subclasses by iodixanol gradient ultracentrifugation. Clin Chem. 2003;49: 1865–72. pmid:14578318
  26. 26. Jenkins AJ, Velarde V, Klein RL, Joyce KC, Phillips KD, Mayfield RK, et al. Native and modified LDL activate extracellular signal-regulated kinases in mesangial cells. Diabetes. 2000;49: 2160–9. pmid:11118021
  27. 27. Kleinveld H a., Hak-Lemmers HLM, Stalenhoef a. FH, Demacker PNM. Improved measurement of low-density-lipoprotein susceptibility to copper- induced oxidation: Application of a short procedure for isolating low-density lipoprotein. Clin Chem. 1992;38: 2066–2072. pmid:1394991
  28. 28. Yokode M, Kita T, Kikawa Y, Ogorochi T, Narumiya S, Kawai C. Stimulated Arachidonate Metabolism during Foam Cell Transformation of Mouse Peritoneal Macrophages with Oxidized Low Density Lipoprotein Electron microscopy oflipoproteins Assayfor lipid peroxides. J Clin Invest. 1988;81: 720–729.
  29. 29. Steinbrecher UP. Oxidation of human low density lipoprotein results in derivatization of lysine residues of apolipoprotein B by lipid peroxide decomposition products. J Biol Chem. 1987;262: 3603–8. pmid:3102491
  30. 30. Schmittgen TD, Livak KJ. Analyzing real-time PCR data by the comparative CT method. Nat Protoc. Nature Publishing Group; 2008;3: 1101–1108.
  31. 31. Holtkamp GM, Van Rossem M, de Vos AF, Willekens B, Peek R, Kijlstra A. Polarized secretion of IL-6 and IL-8 by human retinal pigment epithelial cells. Clin Exp Immunol. 1998;112: 34–43. pmid:9566787
  32. 32. Arnaoutova I, Kleinman HK. In vitro angiogenesis: endothelial cell tube formation on gelled basement membrane extract. Nat Protoc. 2010;5: 628–635. pmid:20224563
  33. 33. Age-Related Eye Disease Study Research Group. A randomized, placebo-controlled, clinical trial of high-dose supplementation with vitamins C and E, beta carotene, and zinc for age-related macular degeneration and vision loss: AREDS report no. 8. Arch Ophthalmol. 2001;119: 1417–36. pmid:11594942
  34. 34. Lee D, Kook S-H, Ji H, Lee S-A, Choi K-C, Lee K-Y, et al. N-acetyl cysteine inhibits H2O2-mediated reduction in the mineralization of MC3T3-E1 cells by down-regulating Nrf2/HO-1 pathway. BMB Rep. Korean Society for Biochemistry and Molecular Biology; 2015;48: 636–41. pmid:26303969
  35. 35. Krilis M, Qi M, Madigan MC, Wong JWH, Abdelatti M, Guymer RH, et al. Nitration of tyrosines in complement factor H domains alters its immunological activity and mediates a pathogenic role in age related macular degeneration. Oncotarget. 2017;8: 49016–49032. pmid:28159936
  36. 36. Sabanayagam C, Lye WK, Januszewski A, Banu Binte Mohammed Abdul R, Cheung GCM, Kumari N, et al. Urinary Isoprostane Levels and Age-Related Macular Degeneration. Investig Opthalmology Vis Sci. 2017;58: 2538. pmid:28492872
  37. 37. Wang AL, Lukas TJ, Yuan M, Neufeld AH. Increased mitochondrial DNA damage and down-regulation of DNA repair enzymes in aged rodent retinal pigment epithelium and choroid. Mol Vis. 2008;14: 644–51. pmid:18392142
  38. 38. Cheng Y-S, Linetsky M, Gu X, Ayyash N, Gardella A, Salomon RG. Light-induced generation and toxicity of docosahexaenoate-derived oxidation products in retinal pigmented epithelial cells. Exp Eye Res. 2018; pmid:30296412
  39. 39. Itabe H. Oxidized low-density lipoprotein as a biomarker of in vivo oxidative stress: from atherosclerosis to periodontitis. J Clin Biochem Nutr. The Society for Free Radical Research Japan; 2012;51: 1–8. pmid:22798705
  40. 40. Palinski W, Ylä-Herttuala S, Rosenfeld ME, Butler SW, Socher SA, Parthasarathy S, et al. Antisera and monoclonal antibodies specific for epitopes generated during oxidative modification of low density lipoprotein. Arteriosclerosis. 1990;10: 325–35. pmid:1693068
  41. 41. Yamada Y, Tian J, Yang Y, Cutler RG, Wu T, Telljohann RS, et al. Oxidized low density lipoproteins induce a pathologic response by retinal pigmented epithelial cells. J Neurochem. 2008;105: 1187–97. pmid:18182060
  42. 42. Pinna A, Zaccheddu F, Boscia F, Carru C, Solinas G. Homocysteine and risk of age-related macular degeneration: a systematic review and meta-analysis. Acta Ophthalmol. 2018;96: e269–e276. pmid:27966830
  43. 43. Singh M, Tyagi SC. Homocysteine mediates transcriptional changes of the inflammatory pathway signature genes in human retinal pigment epithelial cells. Int J Ophthalmol. 2017;10: 696–704. pmid:28546923
  44. 44. Sibrian-Vazquez M, Escobedo JO, Lim S, Samoei GK, Strongin RM. Homocystamides promote free-radical and oxidative damage to proteins. Proc Natl Acad Sci U S A. 2010;107: 551–4. pmid:20080717
  45. 45. Jakubowski H, Głowacki R. Chemical biology of homocysteine thiolactone and related metabolites. Adv Clin Chem. 2011;55: 81–103. pmid:22126025
  46. 46. McCully KS. Chemical pathology of homocysteine. I. Atherogenesis. Ann Clin Lab Sci. 1993;23: 477–93. pmid:8291902
  47. 47. Barathi S, Angayarkanni N, Pasupathi A, Natarajan SK, Pukraj R, Dhupper M, et al. Homocysteinethiolactone and paraoxonase: novel markers of diabetic retinopathy. Diabetes Care. 2010;33: 2031–7. pmid:20551012
  48. 48. Nowotny K, Jung T, Höhn A, Weber D, Grune T. Advanced glycation end products and oxidative stress in type 2 diabetes mellitus. Biomolecules. Multidisciplinary Digital Publishing Institute (MDPI); 2015;5: 194–222. pmid:25786107
  49. 49. Chan C-M, Huang D-Y, Huang Y-P, Hsu S-H, Kang L-Y, Shen C-M, et al. Methylglyoxal induces cell death through endoplasmic reticulum stress-associated ROS production and mitochondrial dysfunction. J Cell Mol Med. 2016;20: 1749–60. pmid:27307396
  50. 50. Penfold PL, Madigan MC, Gillies MC, Provis JM. Immunological and aetiological aspects of macular degeneration. Prog Retin Eye Res. 2001;20: 385–414. pmid:11286898
  51. 51. Spindler J, Zandi S, Pfister IB, Gerhardt C, Garweg JG. Cytokine profiles in the aqueous humor and serum of patients with dry and treated wet age-related macular degeneration. Jablonski MM, editor. PLoS One. 2018;13: e0203337. pmid:30157273
  52. 52. Nassar K, Grisanti S, Elfar E, Lüke J, Lüke M, Grisanti S. Serum cytokines as biomarkers for age-related macular degeneration. Graefe’s Arch Clin Exp Ophthalmol. 2015;253: 699–704. pmid:25056526
  53. 53. Doyle SL, Campbell M, Ozaki E, Salomon RG, Mori A, Kenna PF, et al. NLRP3 has a protective role in age-related macular degeneration through the induction of IL-18 by drusen components. Nat Med. Nature Publishing Group; 2012;18: 791–798. pmid:22484808
  54. 54. Inoue M, Itoh H, Tanaka T, Chun TH, Doi K, Fukunaga Y, et al. Oxidized LDL regulates vascular endothelial growth factor expression in human macrophages and endothelial cells through activation of peroxisome proliferator-activated receptor-gamma. Arterioscler Thromb Vasc Biol. 2001;21: 560–6. pmid:11304473
  55. 55. Maeda M, Yamamoto I, Fujio Y, Azuma J. Homocysteine induces vascular endothelial growth factor expression in differentiated THP-1 macrophages. Biochim Biophys Acta—Gen Subj. 2003;1623: 41–46.
  56. 56. Riazy M, Chen JH, Steinbrecher UP. VEGF secretion by macrophages is stimulated by lipid and protein components of OxLDL via PI3-kinase and PKCζ activation and is independent of OxLDL uptake. Atherosclerosis. 2009;204: 47–54. pmid:18789802
  57. 57. Pertyńska-Marczewska M, Kiriakidis S, Wait R, Beech J, Feldmann M, Paleolog EM. Advanced glycation end products upregulate angiogenic and pro-inflammatory cytokine production in human monocyte/macrophages. Cytokine. 2004;28: 35–47. pmid:15341924
  58. 58. Sakurai E, Anand A, Ambati BK, van Rooijen N, Ambati J. Macrophage depletion inhibits experimental choroidal neovascularization. Invest Ophthalmol Vis Sci. 2003;44: 3578–85. pmid:12882810
  59. 59. Espinosa-Heidmann DG, Suner IJ, Hernandez EP, Monroy D, Csaky KG, Cousins SW. Macrophage depletion diminishes lesion size and severity in experimental choroidal neovascularization. Investig Ophthalmol Vis Sci. 2003;44: 3586–3592.
  60. 60. Zandi S, Nakao S, Chun K-H, Fiorina P, Sun D, Arita R, et al. ROCK-Isoform-Specific Polarization of Macrophages Associated with Age-Related Macular Degeneration. Cell Rep. 2015;10: 1173–1186. pmid:25704819
  61. 61. Bourquain D, Nitsche A. Cowpox virus but not Vaccinia virus induces secretion of CXCL1, IL-8 and IL-6 and chemotaxis of monocytes in vitro. Virus Res. 2013;171: 161–167. pmid:23207068
  62. 62. Yan G, Jiang S, Yu L, Liu S. Oxidized low density lipoprotein (oxLDL) promotes mitochondrial dysfunction and induces apoptosis in retinal pigmented epithelium cells. Int J Clin Exp Pathol. 2017;10: 1619–1626.
  63. 63. Zhang Z, Wei C, Zhou Y, Yan T, Wang Z, Li W, et al. Homocysteine Induces Apoptosis of Human Umbilical Vein Endothelial Cells via Mitochondrial Dysfunction and Endoplasmic Reticulum Stress. Oxid Med Cell Longev. 2017;2017: 1–13. pmid:28630659
  64. 64. Lan K-C, Chiu C-Y, Kao C-W, Huang K-H, Wang C-C, Huang K-T, et al. Advanced Glycation End-Products Induce Apoptosis in Pancreatic Islet Endothelial Cells via NF-κB-Activated Cyclooxygenase-2/Prostaglandin E2 Up-Regulation. Drossopoulou G, editor. PLoS One. 2015;10: e0124418. pmid:25898207
  65. 65. Yating Q, Yuan Y, Wei Z, Qing G, Xingwei W, Qiu Q, et al. Oxidized LDL induces apoptosis of human retinal pigment epithelium through activation of ERK-Bax/Bcl-2 signaling pathways. Curr Eye Res. 2015;40: 415–22. pmid:24956392
  66. 66. Ferlazzo N, Condello S, Currò M, Parisi G, Ientile R, Caccamo D. NF-kappaB activation is associated with homocysteine-induced injury in Neuro2a cells. BMC Neurosci. 2008;9: 62. pmid:18606001
  67. 67. Wang X, Sun Y, Yang H, Lu Y, Li L. Oxidized Low-Density Lipoprotein Induces Apoptosis in Cultured Neonatal Rat Cardiomyocytes by Modulating the TLR4/NF-κB Pathway. Sci Rep. Nature Publishing Group; 2016;6: 27866. pmid:27279424
  68. 68. Ryu J, Kwon M-J, Nam T-J. Nrf2 and NF-κB Signaling Pathways Contribute to Porphyra-334-Mediated Inhibition of UVA-Induced Inflammation in Skin Fibroblasts. Mar Drugs. 2015;13: 4721–32. pmid:26264001
  69. 69. Jasna JM, Anandbabu K, Bharathi SR, Angayarkanni N. Paraoxonase enzyme protects retinal pigment epithelium from chlorpyrifos insult. PLoS One. 2014;9: e101380. pmid:24979751
  70. 70. Ghosh S, Shang P, Terasaki H, Stepicheva N, Hose S, Yazdankhah M, et al. A Role for βA3/A1-Crystallin in Type 2 EMT of RPE Cells Occurring in Dry Age-Related Macular Degeneration. Investig Opthalmology Vis Sci. 2018;59: AMD104. pmid:30098172