About this Journal Submit a Manuscript Table of Contents
ISRN Dermatology
Volume 2013 (2013), Article ID 825180, 12 pages
http://dx.doi.org/10.1155/2013/825180
Research Article

Emptying of Intracellular Calcium Pool and Oxidative Stress Imbalance Are Associated with the Glyphosate-Induced Proliferation in Human Skin Keratinocytes HaCaT Cells

Proteomics Laboratory, Indian Institute of Toxicology Research (CSIR), Mahatma Gandhi Marg, Lucknow, Uttar Pradesh 226001, India

Received 16 May 2013; Accepted 17 July 2013

Academic Editors: C. Feliciani and A. Zalewska

Copyright © 2013 Jasmine George and Yogeshwer Shukla. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

We demonstrated that glyphosate possesses tumor promoting potential in mouse skin carcinogenesis and SOD 1, calcyclin (S100A6), and calgranulin B (S100A9) have been associated with this potential, although the mechanism is unclear. We aimed to clarify whether imbalance in between levels and oxidative stress is associated with glyphosate-induced proliferation in human keratinocytes HaCaT cells. The levels, ROS generation, and expressions of G1/S cyclins, IP3R1, S100A6, S100A9, and SOD 1, and apoptosis-related proteins were investigated upon glyphosate exposure in HaCaT cells. Glyphosate (0.1 mM) significantly induced proliferation, decreases , and increases ROS generation in HaCaT cells, whereas antioxidant N-acetyl-L-cysteine (NAC) pretreatment reverts these effects which directly indicated that glyphosate induced cell proliferation by lowering levels via ROS generation. Glyphosate also enhanced the expression of G1/S cyclins associated with a sharp decrease in G0/G1 and a corresponding increase in S-phases. Additionally, glyphosate also triggers S100A6/S100A9 expression and decreases IP3R1 and SOD 1 expressions in HaCaT cells. Notably, Ca2+ suppression also prevented apoptotic related events including Bax/Bcl-2 ratio and caspases activation. This study highlights that glyphosate promotes proliferation in HaCaT cells probably by disrupting the balance in between levels and oxidative stress which in turn facilitated the downregulation of mitochondrial apoptotic signaling pathways.

1. Introduction

Glyphosate, “an organophosphate herbicide,” is the active component of Roundup and considered being innocuous whether alone or in combination with its formulation products such as surfactants under regular usage or chronic exposure in earlier testing approach in humans [1, 2]. However, lately acute toxic activity of glyphosate at lethal concentration has been demonstrated in fish or other aquatic organisms [3, 4]. Some case-control studies suggested an association between glyphosate use and the risk of non-Hodgkin lymphoma among men [5].

The cellular reply to carcinogens/toxicants is intricate, and considerable effort is put into defining the network of proceedings going on in the cell to preserve genomic stability and avert carcinogenesis. Intracellular Ca2+ signaling is vital in the regulation of multiple cellular processes, including development, proliferation, secretion, gene activation, and cell death [68]. The development of these Ca2+ signals is reliant on many cellular Ca2+-binding and Ca2+-transporting proteins, existing in the several cell compartments of which the endoplasmic reticulum (ER) forms the main intracellular Ca2+ store [9]. The S100 family is Ca2+-binding proteins comprises around 20 genes that are positioned in a cluster on chromosome 1q21 [10]. Expression of several S100 proteins appears to be transformed in different types of cancers [11]. Particularly, calcyclin (S100A6) and calgranulin B (S100A9) containing 2 EF-hand Ca2+-binding motifs are presently enticing ample attention for their extensive variety of potential intracellular along with extracellular functions [12]. For instance, both proteins have been proposed to be involved in the regulation of cell proliferation, apoptosis, and motility through Ca2+-dependent signaling pathways [13]. Likewise, both of them have been defined to play a part in the pathogenesis of epidermal disease involving melanoma or epithelial skin cancer and inflammation [14]. The expression pattern of S100A6 and S100A9 expressions was found to be considerably enhanced in some tumor tissues like hepatocellular carcinoma [15], lung cancer [16], colorectal cancer [17], and melanoma [18].

Modification in the ionized intracellular Ca2+ concentration has been associated with the production of reactive oxygen species (ROS) [19]. ROS (, hydrogen peroxide (H2O2), ROOH, HO, etc.) are commonly considered as toxicants that persuade numerous toxic effects, like cell dysfunction, death, or malignant transformation. Oxidative stress is the consequence of the disparity between ROS generation and the cellular antioxidant capacity. It is well-documented that substantial oxidative stress brings out severe harm to lipids, proteins, sugars, and nucleic acid bases, which compromises cell viability and functions [2022]. In experimental models by means of cell lines, it was displayed that ROS generation and consequent oxidative stress add to cancer progress through arrange of interconnected signals [23]. To bestow, shield against the oxidative stress, the skin is equipped with quite a few enzymatic antioxidants, like superoxide dismutase (SOD), catalase, and many peroxidases [24]. SOD is a tumor suppressor protein that upsurges the dismutation rate of superoxide anion () to H2O2 by 3 to 4 orders of magnitude over unstructured dismutation and prevents cancer cell growth in vitro [25, 26]. CuZnSOD (SOD 1) is an Mr 32,000 dimeric SOD family protein that is confined in the cytoplasm [27]. Reports suggest that SOD 1 might be involved in cancer cell invasion and metastasis [28, 29].

Previously, we have reported that glyphosate potentially causes tumor promotion in mouse skin carcinogenesis and S100A6, S100A9, and SOD 1 are associated with this tumor promotion [30]. However, the mechanism behind glyphosate-induced tumor promotion is not fully understood. This prompted us to explore the possibility whether deregulation of Ca2+ homeostasis and oxidative stress are playing a role in the proliferation activity of glyphosate. For this, we have studied the underlying mechanism using human skin keratinocyte, HaCaT, cells as an in vitro model. These cells were derived from a spontaneously immortalized human keratinocyte. They are a nontumorigenic epidermal cell line that exhibits many of the morphological and functional properties of normal human keratinocytes. The use of HaCaT cells has the good advantage of providing an almost unlimited supply of identical cells, assuring high reproducibility; this cellular model also possesses the enzymatic equipment to bioactivated or detoxifies xenobiotics [31].

2. Materials and Methods

2.1. Chemicals

The commercial formulation of the herbicide glyphosate (N-phosphonomethyl-glycine) Roundup Original (glyphosate 41%, polyethoxethyleneamine (POEA) 15%—Monsanto Company, St. Louis, MO, USA) was used. It contains glyphosate 360 g/L (acid equivalent) present as the isopropylamine salt and was procured from local market. 2′,7′-Dichlorodihydrofluorescein diacetate dye (H2DCF-DA), propidium iodide (PI), 3[4-Dimethylthiazol-2-yl]-2-5-diphenyl tetrazolium bromide (MTT), 4,6-diamidino-2-phenylindole (DAPI), and N-acetyl-L-cysteine (NAC) were purchased from Sigma Chemical Company (St. Louis, CA, USA). Cyclin D1, cdk 4, cdk 6, cyclin E, cdk 2, caspase 3, caspase 9, cytochrome c, apoptotic protease-activating factor-1 (Apaf-1), and β-actin antibodies were procured from Cell Signaling Technology (Beverly, MA, USA). Bax, Bcl-2, PCNA (proliferating cell nuclear antigen), BrdU (5-bromo-2′-deoxyuridine), 1 inositol-1,4,5-trisphosphate receptor type 1 (IP3R1), S100A6, S100A9, and SOD1 antibodies were procured from Santa Cruz Biotechnology Inc., Europe. Fluorescein isothiocyanate (FITC), rhodamine, and horseradish peroxidase (HRP) conjugated anti-mouse/anti-rabbit secondary antibodies were procured from Bangalore Genei (Bangalore, India) and Cell Signaling Technology, Inc. (Danvers, MA, USA), respectively. The polyvinylidene fluoride (PVDF) membrane was obtained from Millipore (Bedford, MA, USA). All other chemicals were of analytical grade of purity and were procured locally.

2.2. Cell Culture

HaCaT cells were procured from National Centre for Cell Science, Pune, India, and cultured in calcium free-Dulbecco’s modified Eagle’s medium (DMEM) (catalog number 21068-028, Invitrogen, Carlsbad, CA, USA) supplemented with 10% chelex-treated fetal bovine serum (FBS), 1% penicillin streptomycin (Gibco Lifetech, Karlsruhe, Germany). Cells were maintained in a humidified atmosphere of 95% air and 5% CO2 at 37 degrees in incubator.

2.3. Cell Proliferation Assay by MTT

To evaluate the dose-response effect of glyphosate on the growth and proliferation of HaCaT cells, the MTT assay was performed as described earlier [32]. Briefly, cells per well were plated in 96-well flat-bottomed microplate and treated with glyphosate (0.01, 0.025, 0.05, 0.1, 0.25, 0.5, and 1 mM) for 24, 48, and 72 h. To address the antiproliferative potential of NAC, HaCaT cells were alone and preincubated with NAC (10 and 20 mM) followed by a 72 h incubation with glyphosate (0.1 mM). After the incubation, the cells were washed twice with PBS, and 200 μL of culture medium containing 5 mg/mL of MTT dye was added to each well and incubated further for 4 h. The medium containing MTT dye was then replaced with 200 μL of dimethyl sulfoxide (DMSO). The plates were then agitated for 10 min, and the optical density (OD) was measured at 540 nm using microplate reader (FLUOstar Omega-BMG Labtech). 12-O-tetradecanoyl-phorbol-13-acetate (TPA) (10 nM) was used as a positive control group.

2.4. Immunofluorescence Studies

HaCaT cells proliferation was examined using immunofluorescence staining for PCNA and BrdU. Briefly, HaCaT cells were incubated with glyphosate (0.01, 0.1 mM) and TPA (10 nM) for 72 h. Then, BrdU (10 mM) was added to the medium, and the cells were incubated for 4 h. This exposure was followed by fixing with 4% paraformaldehyde in PBS for 7 min, permeabilization with 0.1% Triton-X-100 in PBS for 7 min, and blocking with 3% BSA in PBS for 1 h with gentle agitation. Further, the cells were incubated with BrdU and PCNA primary antibody for overnight and secondary rhodamine antibody for BrdU and FITC antibody for PCNA at room temperature for 1 h each. The cells were then washed in PBS and counterstained with DAPI. Fluorescence microscopy was performed using olympus IX51 (Olympus America Inc., Center Valley, PA, USA), and images were acquired with the help of software Image-Pro Express.

2.5. Treatment of Cells

Glyphosate stock solution (1 mM in the medium) was prepared in the medium and diluted further in fresh medium to achieve desired final concentration for treatment of cells. Cells that served as vehicle controls were incubated with the medium only. The cells were harvested by trypsinization, washed twice with cold PBS to remove residual medium, and processed as per the requirement of the following assays.

2.6. Intracellular Ca2+ Measurement

Intracellular Ca2+ concentration was measured with the Ca2+ indicator dye Fura-2 AM (Sigma Aldrich, USA). Cells were seeded at a density of 16000 cells/well in completed growth medium in a 96-well plate. Next day, they were loaded with Fura-2 AM in loading solution (125 mM NaCl, 5 mM KCl, 1.2 mM MgSO4, 1.2 mM KH2PO4, 2 mM CaCl2, 6 mM Glucose, and 25 mM Hepes (pH-7.0)) at 37°C under CO2 incubator for 30 min. Excess dye was removed by rinsing twice with wash buffer (NaCl, KCl, NaHCO3, and Glucose). Thereafter, cells were treated with NAC (20 mM), glyphosate (0.1 mM), and TPA (10 nM) for 6 h, respectively, harvested, and washed twice with wash buffer. For NAC treatment, cells were preincubated with 20 mM NAC before treating with the same concentration of glyphosate and TPA. Fluorescence was monitored every 10 min at the excitation wavelength of 355 and 380 nm and the emission wavelength of 510 nm at each time point (0–6 h) by microplate reader (FLUOstar Omega-BMG Labtech). All results showed are representative experiments from three separate experiments under the same conditions and by a same procedure at each time point. To convert fluorescent values into absolute Ca2+ concentration, calibration was performed at the end of each experiment. The concentration of intracellular Ca2+ concentration was calculated using the following formula: where Kd is the dissociation constant of the Ca2+-bound Fura-2 AM complex (224 nM/L), and is excitation obtained at the ratio generated by 355/380. corresponds to the maximum fluorescence obtained by treating cells with 0.1% Triton X-100, and represents the minimum fluorescence of the cells treated with 5 mM EGTA.

2.7. Measurement of ROS Generation

ROS generation was monitored by using H2DCFH-DA as described by earlier [33] with slight modifications. Briefly, cells were seeded at a density of cells/well in a 96-well plate, respectively. The next day, cells were treated with N-acetyl-cysteine (NAC) (20 mM), glyphosate (0.1 mM), TPA (10 nM), and H2O2 (100 mM) for 24 h followed by incubation with 10 μM H2DCFH-DA at 37°C for 30 min in dark. For NAC treatment, cells were preincubated with 20 mM NAC for 1 h after synchronization before treating with the same concentration of glyphosate, TPA, and H2O2. Fluorescence was measured through a spectrofluorometer by using 507 nm as excitation and 530 nm as emission wavelengths. For each experiment, fluorometric measurements were performed in triplicate, and data is presented as the percentage of vehicle control cells.

2.8. Cell-Cycle Analysis

For cell-cycle analysis, the cells were prepared as described earlier [34]. Briefly, vehicle, positive control, and glyphosate (0.1 mM) exposed cells (for 24 h) were washed with PBS and centrifuged at 200 ×g for 10 min at 4°C. The pellet was fixed in 1 mL of  70% ice-cold ethanol for 30 min and resuspended in 50 μg/mL PI with RNase A (100 μg/mL) followed by incubation for 30 min in dark. The samples were acquired and analyzed on flow cytometer using “CellQuest” software.

2.9. Total Cell Lysate Preparation

Following glyphosate (0.1 mM) and TPA (10 nM) treatment to the cells for 24, 48, and 72 h, the medium was aspirated, and the cells were washed twice with cold PBS (10 mM, pH 7.4). Ice-cold lysis buffer (50 mM Tris-HCl, 150 mM NaCl, 1 mM EGTA, 1 mM EDTA, 20 mM NaF, 100 mM Na3VO4, 0.5% NP-40, 1% Triton X-100, 1 mM PMSF, 10 μg/mL aprotinin, 10 μg/mL leupeptin, and pH 7.4) was added to the plates, which were then placed over ice for 30 min [33]. The cells were scraped, and the lysate was collected in a microfuge tube. The lysates were cleared by centrifugation at 14000 ×g for 15 min at 4°C, and the supernatant (total cell lysate) was either used immediately or stored at −80°C.

2.10. Immunoblotting

Immunoblotting was carried in the total cell lysates of HaCaT cells. Proteins (50 μg) were resolved on 10–12% SDS-PAGE, electroblotted onto PVDF membranes, and incubated with antibodies of cyclin D1,cdk 4, cdk 6, cyclin E, cdk 2, IP3R, S100A6, S100A9, SOD 1, Bax, Bcl-2, Apaf-1, cytochrome c, caspases 3, 9, and β-actin. HRP-conjugated secondary antibodies and chemiluminescence kit (Millipore, USA) were used for detection. Proteins expression was visualized by Versa Doc 4000 MP Imaging System (Bio-Rad Hercules, CA, USA). The intensity of the bands normalized to the band of β-actin was measured using software UNSCAN-IT automated digital system version 5.1 (Orem, USA) and then given in terms of calculated quantitative fold change with respect to control.

2.11. Statistical Analysis

The data were analyzed to obtain mean values and standard deviation for all treated and vehicle control samples, which were subjected to statistical comparison using student- test; was considered as significant.

3. Results

3.1. Glyphosate-Induced Proliferation in HaCaT Cells

The proliferation rate of HaCaT cells exposed to different concentrations (0.01, 0.025, 0.05, 0.1, 0.25, 0.5, and 1 mM) of glyphosate was evaluated for 24, 48, and 72 h using the MTT assay (Figure 1(a)). Glyphosate at 0.1 mM and lower concentration promoted the growth of HaCaT cells, whereas doses higher than 0.1 mM reduced cell growth in time dependent manner. A significant increase in proliferation was observed in cells exposed to glyphosate at 72 hrs of exposure as compared to the number of viable cells in control at all concentrations except the highest doses (0.25, 0.5, and 1 mM); (Figure 1(a)).

fig1
Figure 1: (a) Proliferation effects of glyphosate on HaCaT cells. Cells were exposed to glyphosate (0.01–1 mM) and positive control, and TPA (10 nM) for 24, 48, and 72 h. (b) Inhibition of glyphosate (0.1 mM) induced cell proliferation after 72 h by a prior treatment of NAC (10 mM and 20 mM). OD values from three separate experiments are shown as mean ± SD. *Increase over vehicle control cells (); **decrease over glyphosate alone treated cells ().

Proliferation induced by glyphosate in the presence of antioxidant NAC was significantly inhibited compared to glyphosate alone and was not significantly different from control incubated with NAC alone, suggesting that ROS may be involved in glyphosate proliferation effect (Figure 1(b)).

Consistently data from fluorescence microscopy showed increased PCNA expression and a high proportion of BrdU stained cells, indicated a significant () increase in cell proliferation rate in glyphosate (0.1 mM) treated HaCaT cells over control cultures (Figure 2). Thus, proliferative dose of 0.1 mM was used further in all assays.

fig2
Figure 2: PCNA and BrdU staining of glyphosate and TPA-treated HaCaT cells. HaCaT cells were treated with glyphosate and TPA and were incubated for 72 h. (a) Cells were fixed, and PCNA was detected by immunofluorescence with an anti-PCNA antibody and FITC-labeled secondary antibody (green color). Pictures with green and blue colors were merged. DNA was stained with DAPI (blue color). (b) Cells were pulsed for 4 h with BrdU, fixed, and detected with an anti-BrdU antibody and rhodamine-labeled secondary antibody (red color). DNA was stained with DAPI (blue color). Pictures with red and blue colors were merged. Histogram represents the relative fluorescence intensity of PCNA and BrdU positive cells expressed as a ratio between control and treated HaCaT cells. For all panels, representative data from mean ± SD of at least three independent experiments are shown. versus control cells.
3.2. Glyphosate Decreases Intracellular Ca2+ Level in HaCaT Cells

To determine whether or not intracellular Ca2+ signals promote cell proliferation, we measured the Ca2+ concentration in vehicle, positive control, glyphosate, and NAC treated HaCaT cells at regular time intervals (0–6 h). was measured with a calcium indicator dye Fura-2 AM. Incubation of cells with glyphosate (0.1 mM) and TPA (10 nM) resulted in a time-dependent decrease of in HaCaT cells as compared with control cells, , whereas NAC increases above control levels (Figure 3(a)). These data suggest that the fall in is due to the decrease Ca2+ influx through cell membrane channels. Though, a rapid increase in fluorescence was detected when antioxidant, NAC was added to the cell suspension. From these results, we hypothesize that pretreatment with NAC might cause the opening of Ca2+ channels, allowing rapid influx of extracellular Ca2+ (Figure 3(b)).

fig3
Figure 3: Measurement of glyphosate-induced changes in intracellular Ca2+ level in HaCaT cells by spectrofluorometry with Fura-2/AM dye. (a) Ca2+ level was measured after treatment with NAC (20 mM), 0.1 mM glyphosate, and 10 nM TPA at 0–6 h. (b) Ca2+ level was measured after a prior treatment with 20 mM NAC. Results are mean ± SD from three independent experiments. *Decrease over control cells (); **increase over control cells ().
3.3. Glyphosate Increases ROS Generation in HaCaT Cells

Next we sought to test whether glyphosate-elevated is mediated by ROS induction, leading to cell proliferation. To this end, HaCaT cells were exposed to 0-0.1 mM glyphosate, 10 nM TPA, and 100 mM H2O2 for 24 h. As shown in Figure 4(a), exposure to glyphosate (0.1 mM) increased maximum ROS levels by approximately 90% in HaCaT cells as compared with vehicle control cells. Additionally, ROS generation was similar in glyphosate and positive controls TPA (~70%) and H2O2 (~80%) treated cells (Figure 4(a)). However, upon pretreatment of the cells with the ROS scavenger NAC in glyphosate (0.1 mM), TPA, and H2O2 treated cells, ROS generation was abrogated to almost 50%, 70%, and 80% respectively, as compared to that in vehicle control cells, (Figure 4(b)). Moreover, NAC (20 mM) alone treatment has no effect on ROS. These results support that NAC is effective in preventing increase in and oxidative stress resulting from exposure to glyphosate in HaCaT cells. Collectively, these results showed that ROS is involved in the elevation of which in turn is a crucial element in the progression of glyphosate-induced cell proliferation.

fig4
Figure 4: Measurement of glyphosate-induced generation of ROS in HaCaT cells. (a) Generation of ROS was measured using the fluorescent dye (5 (and 6)-chloromethyl-20, 70-dichlorodihydro-fluorescein diacetate acetyl ester) after treatment of HaCaT cells with vehicle alone, NAC (20 mM), (0.01–0.1 mM) glyphosate, and 10 nM TPA. (b) Inhibition of ROS generation after a prior treatment of NAC. Data are expressed as mean ± SD of three independent experiments. *Increase in ROS generation versus control cells (); **decrease in ROS generation versus control cells ().
3.4. Glyphosate-Induced Growth of HaCaT Cells in S-Phase of Cell Cycle and Elevates Expression of G1/S-Phase’s Proteins

To determine whether glyphosate-induced cell-cycle progression of HaCaT cells, cell-cycle distribution was analyzed by flow cytometry after exposure to glyphosate for 24 h. Analysis of the cell cycle distributions of HaCaT cells after exposure to glyphosate (0.1 mM) and TPA (10 nM) showed that more cells were in the S-phase of the cell cycle as compared with untreated control cells accompanied by a significant decrease in the G0/G1-phase (Figures 5(a) and 5(b)). To determine if glyphosate-induced growth of HaCaT cells was due to increased activation of the cell-cycle machinery, expression of cell-cycle regulatory proteins was examined using immunoblot assay. Treatment of cells with glyphosate (0.1 mM) and TPA resulted in a time-dependent increase in the expression of cyclin D1, cdk4, cdk6, cyclin E, and cdk2 as compared with vehicle control cells (72 h) (Figure 5(c)). Collectively, these results demonstrate that glyphosate induces expression of G1/S phase’s proteins and enhances cell proliferation.

fig5
Figure 5: Effect of glyphosate on cell-cycle progression and G1/S-phase proteins in HaCaT cells. Cultured cells were treated with (a) vehicle, glyphosate (0.1 mM), and TPA (10 nM). 24 h later, cell cycle was analyzed by flow cytometry. (b) Quantitative assessment of the percentage of HaCaT cells in G1/S-phases, as indicated by propidium iodide (PI). (c) Immunoblot of G1-S-phase cell-cycle-associated proteins in HaCaT cells after treatment with glyphosate and TPA for 24, 42, and 72 h. All results represent the average of three independent experiments ± S.D. * compared with the vehicle control.
3.5. Glyphosate Modulates Ca2+ Release Channel, Ca2+ Binding, Oxidative Stress, and Apoptosis-Related Proteins

In clarifying the mechanism of glyphosate-induced proliferation in HaCaT cells, we further examined the expression of IP3R1 isoform of IP3Rs-Ca2+ release channel, the proteins that bind Ca2+ (S100A6 and S100A9), reduce oxidative stress (SOD 1), and regulate apoptosis (Bax, Bcl-2, cytochrome C, apaf-1, caspases 3, 9) after glyphosate (0.1 mM) and TPA (10 nM) treatment at 24, 48, and 72. In glyphosate treated cells, we found the expression of IP3R1 to be hardly detectable at all-time intervals (Figure 6(a)). Little immunoreactivity for S100A6 and S100A9 was visible in vehicle control cultures (72 h) (Figure 6(a)), but dramatic increase of S100A6 and S100A9 expressions was found at designated time points after treatment of glyphosate and TPA (Figure 6(a)). Significant decrease in expression of SOD 1 in glyphosate and TPA exposed cells was also seen in time dependent manner (Figure 6(a)). The immunoreactivity for Bcl-2 was also markedly increased at the same time points posttreatments (Figure 6(b)), whereas Bax, cytochrome C, apaf-1, and caspases 3, 9 expressions were significantly reduced at all-time points after treatment of glyphosate (Figure 6(b)).

fig6
Figure 6: Western blots showing the proliferative effect of glyphosate (0.1 mM) and TPA (10 nM) on the expression levels of (a) Ca2+ binding and oxidative stress and (b) apoptosis-related proteins in HaCaT cells for 24, 42, and 72 h. The bands shown here are from a representative experiment repeated three times with similar results. Equal loading was confirmed by stripping the immunoblot and reprobing it for β-actin. Quantitative fold change was calculated in respect to control on the basis of pixel density measured by UNSCAN-IT software.

4. Discussion

The low reported acute toxicity and short environmental persistence of the herbicide-glyphosate have allowed its worldwide usage in agriculture, even though numerous genotoxic effects have been reported [3537]. We have previously reported that glyphosate potentially causes tumor promotion in two-stage mouse skin carcinogenesis model, and S100A6, S100A9 (Ca2+-regulating proteins), SOD 1 (oxidative stress-related protein) are associated with this tumor promotion [30]. However, the molecular mechanism, how glyphosate contributes in tumor promotion, and regulation of S100A6, S100A9, and SOD 1 remain elusive and require more detailed analysis of the mechanism.

In order to clarify the mode of tumorigenic action of glyphosate, we used human skin keratinocytes HaCaT cells as an in vitro model and observed that the imbalance between Ca2+ homeostasis and cellular oxidative stress is mainly responsible for glyphosate induced hyperproliferation of HaCaT cells. Using cell proliferation assay, PCNA, and BrdU staining, the effect of glyphosate on cellular proliferation in HaCaT cells was examined. Glyphosate (0.1 mM) significantly increases cell proliferation accompanied with increased PCNA as well as BrdU positivity further suggested its carcinogenic potential (Figures 1 and 2).

Calcium signalling plays a pivotal role in the regulation of the growth, differentiation, and apoptosis of many kinds of cells including epidermal keratinocytes [38]. Ca2+ concentrations may vary with time, even may oscillate (Ca2+ influx from intracellular stores and subsequent extracellular Ca2+ entry) offering a room for somewhat diverse outcomes such as increased cell proliferation versus differentiation and viability versus death in different types of cells including tumor cells [39]. Considering the importance of Ca2+ level in inducing cell proliferation, we measured changes in intracellular Ca2+ concentration in glyphosate treated HaCaT cells, respectively, at regular time intervals. Our data demonstrated that control cells maintained while glyphosate significantly decreases in a time dependent manner at proliferation inducing dose for HaCaT cells (Figure 3). Our results are consistent with the findings of Gniadecki and Gajkowska [38] suggesting that emptying intracellular Ca2+ stores in keratinocytes (e.g., by a selective blocker of calcium pump, thapsigargin) facilitates basal cell carcinomas or squamous cell carcinomas development. Thus, these results suggest that glyphosate promotes proliferation via modulation of Ca2+ levels.

Previously, in vitro studies had addressed that glyphosate facilitates oxidative stress [37, 40], and in this study, we confirmed that glyphosate treated HaCaT cells differ from vehicle control cells in the oxidative stress level. The levels of ROS production in glyphosate, TPA, and H2O2 treated cells were significantly higher than those found in control cells (Figure 4(a)). As oxidative stress and changes in are intimately related, thus, in order to verify the correlation between modifications and the effects of oxidative stress we used NAC, a potent antioxidant which has been demonstrated to be able to promote apoptosis in several cell lines [41, 42]. The antiproliferative effects of 20 mM NAC by reducing ROS have been shown in glioma cells [43]. Here, we observed a substantial decrease in cell proliferation followed by elevation of level and decrease in ROS generation during pretreatment with NAC (20 mM) suggesting ROS has a significant role in the elevation of which in turn is a crucial element in the progression towards cell death as most endonucleases require the presence of Ca2+ to cleave DNA strands. These results imply that glyphosate induced cell proliferation by lowering levels was mediated by ROS generation. Therefore, the molecular mechanism for glyphosate induced cell proliferation involves an imbalance in between Ca2+ homeostasis and element of oxidative stress, that is, ROS.

Cell-cycle dysregulation is a hallmark of tumor cells and human cancers. The cell-cycle checkpoints failure causes genetic instability and consequent growth of cancers from the affected cell [44]. Calcium release or decrease in stores might allow the progression from G0 to G1 of cell cycle [45]. Further in this study, we examined the effect of glyphosate on the progression of cell cycle. As shown in Figures 5(a) and 5(b), glyphosate treatment increases cell growth from G1- to S-phase of the cell-cycle as compared with vehicle control cells. Moreover, the results of the present study indicate that glyphosate caused cell cycle acceleration together with an increase in cyclin D1/cdk4, cyclin D1/cdk6, and cyclin E/cdk2, which are involved in cell-cycle progression from G1- to S-phase (Figure 5(c)). Thus, the data clearly showed that glyphosate accumulated cells in S-phase of the cell-cycle concomitant with a decrease in levels and increase in ROS generation.

Next, we investigated the expression of the proteins that regulate the levels, oxidative stress, and apoptosis. The results of the present study showed a significant increase in two Ca2+ binding proteins, S100A6, and S100A9 (Figure 6(a)). In the past, we studied alterations in global protein expression using samples of mouse skin treated with glyphosate and the tumor promoter TPA, which is a potent activator of keratinocyte proliferation [46], epidermal hyperplasia and dermal inflammation [47], and we found strong upregulation of S100A6 and S100A9 [30]. More recently, strong upregulation of both proteins was also reported by us in HaCaT cells upon mancozeb (fungicide) exposure [48]. Numerous recent reviews focused on the extracellular function of S100A6/A9 and its presumed impact on pathological processes such as acute and chronic inflammations or carcinogenesis [4951]. Ca2+ binding prompts a conformational variation in the S100A6 molecule which in result raises its total hydrophobicity and lets the target proteins and transduction of Ca2+ signals collaborate [52]. However, the crosstalk between Ca2+ level changes and these Ca2+ binding proteins in cancer progression remains elusive. Glyphosate treatment also significantly reduced expression of antioxidant SOD 1 protein in HaCaT cells thus can be associated with stimulation of oxidative stress (Figure 6(a)). These results suggest that glyphosate treatment could cause intracellular Ca2+ imbalance, induce cellular oxidative stress, and modify S100A6/A9 and Cu/Zn-SOD 1 expressions, a phenomenon that may contribute to the mechanisms involved in HaCaT cell proliferation.

In a cellular system, one of the two foremost ways of Ca2+ discharge from the Ca2+ store is the IP3Rs, the other being ryanodine receptor (RyR). Essential to an understanding of Ca2+ signaling hence is gratitude of the control of IP3Rs-mediated Ca2+ release [53, 54]. Three mammalian isoforms of IP3R exist, namely, IP3R1, IP3R2, and IP3R3 known to play a key role in promoting different signaling prospects during changes in Ca2+ levels. One intriguing factor is the proximity of ER to mitochondria that may facilitate the mitochondrial overload of Ca2+ released from the IP3Rs with certain apoptotic stimuli, triggering the opening of the mitochondrial permeability transition pore and the release of apoptotic signaling molecules, such as cytochrome c and apoptosis-inducing factor, which leads to the activation of caspases [55, 56]. Moreover, several key components of apoptotic cascades, such as cytochrome c [57] and anti-apoptosis proteins Bcl-2 [58, 59] and Bcl-XL [60], have been reported to interact with the internal coupling domain and/or the COOH-terminal tail of IP3R and enhance the Ca2+ release activity of IP3Rs during apoptosis. It has been shown that less apoptosis occurs in cells in which IP3R1 expression was reduced or wholly silenced [61]. Similarly, in our case the decrease in the level of IP3R1 also observed upon glyphosate exposure in HaCaT cells thus prevented cell death [62]. Furthermore, in the cancer cells the amplified appearance of antiapoptotic members of the Bcl-2 family of proteins or reduced appearance of the proapoptotic proteins like Bax or Bak can shield these cells from apoptosis by controlling signals [63, 64]. This mechanism was also observed in our case as we found a significant increase in Bcl-2 and decrease in Bax proteins simultaneously with a decrease in levels (Figure 6). The rise of has been demonstrated to cause mitochondrial inner transmembrane potential collapse and release of cytochrome c, activation of caspase 3, and then apoptosis [41]. In contrast, in the present study, we found that lowering with glyphosate treatment suppressed the activation of caspases and thereby possibley preventing apoptosis. The results of our studies can be summarized in a schematic presentation (Figure 7).

825180.fig.007
Figure 7: Proposed itinerary for glyphosate-induced proliferation in human skin keratinocytes HaCaT cells.

5. Conclusion

In conclusion, in this study, we demonstrated that glyphosate may possibly exert proliferative effect in HaCaT cells by activating Ca2+ binding proteins to promote the imbalance of intracellular Ca2+ homeostasis and lessen SOD1 to increase ROS generation. This effect was partially reversed by treatment with antioxidant NAC indicating connections between oxidative stress and hypocalcaemia. Reduced Ca2+ levels enhance Bcl-2 and decrease Bax, subsequently leading to decrease in cytochrome c to stimulate further decrease of caspase 3 via the downregulation of IP3R1 level, thus halting apoptosis. The present study for the first time provides insight into the mechanism of glyphosate-induced neoplastic potential in mammalian skin system.

Conflict of Interests

All authors report that there is no conflict of interests.

Acknowledgments

This work was funded from Task Force Project NWP-17 supported by the Council of Scientific and Industrial Research, New Delhi, India, and provided fellowship to Jasmine George. The authors are thankful to Dr. K. C. Gupta, Director, IITR, Lucknow, for his keen interest in the study. The authors are thankful to Dr. A. B. Pant for his kind cooperation and assistance in conducting the study.

References

  1. J. Malik, G. Barry, and G. Kishore, “The herbicide glyphosate,” Biofactors, vol. 2, no. 1, pp. 17–25, 1989. View at Scopus
  2. G. M. Williams, R. Kroes, and I. C. Munro, “Safety evaluation and risk assessment of the herbicide Roundup and its active ingredient, glyphosate, for humans,” Regulatory Toxicology and Pharmacology, vol. 31, no. 2, part 1, pp. 117–165, 2000. View at Publisher · View at Google Scholar · View at Scopus
  3. R. B. Bringolf, W. G. Cope, S. Mosher, M. C. Barnhart, and D. Shea, “Acute and chronic toxicity of glyphosate compounds to glochidia and juveniles of Lampsilis siliquoidea (Unionidae),” Environmental Toxicology and Chemistry, vol. 26, no. 10, pp. 2094–2100, 2007. View at Publisher · View at Google Scholar · View at Scopus
  4. L. Glusczak, V. L. Loro, A. Pretto et al., “Acute exposure to glyphosate herbicide affects oxidative parameters in piava (Leporinus obtusidens),” Archives of Environmental Contamination and Toxicology, vol. 61, no. 4, pp. 624–630, 2011. View at Publisher · View at Google Scholar · View at Scopus
  5. A. J. de Roos, S. H. Zahm, K. P. Cantor et al., “Integrative assessment of multiple pesticides as risk factors for non-Hodgkin's lymphoma among men,” Occupational and Environmental Medicine, vol. 60, no. 9, article E11, 2003. View at Scopus
  6. H. Hennings, D. Michael, C. Cheng, P. Steinert, K. Holbrook, and S. H. Yuspa, “Calcium regulation of growth and differentiation of mouse epidermal cells in culture,” Cell, vol. 19, no. 1, pp. 245–254, 1980. View at Publisher · View at Google Scholar
  7. A. H. Lichtman, G. B. Segel, and M. A. Lichtman, “The role of calcium in lymphocyte proliferation. (An interpretive review),” Blood, vol. 61, no. 3, pp. 413–422, 1983. View at Scopus
  8. M. Whitaker and R. Patel, “Calcium and cell cycle control,” Development, vol. 108, no. 4, pp. 525–542, 1990. View at Scopus
  9. M. J. Berridge, P. Lipp, and M. D. Bootman, “The versatility and universality of calcium signalling,” Nature Reviews Molecular Cell Biology, vol. 1, no. 1, pp. 11–21, 2000. View at Scopus
  10. A. Mueller, T. Bächi, M. Höchli, B. W. Schäfer, and C. W. Heizmann, “Subcellular distribution of S100 proteins in tumor cells and their relocation in response to calcium activation,” Histochemistry and Cell Biology, vol. 111, no. 6, pp. 453–459, 1999. View at Publisher · View at Google Scholar
  11. I. Salama, P. S. Malone, F. Mihaimeed, and J. L. Jones, “A review of the S100 proteins in cancer,” European Journal of Surgical Oncology, vol. 34, no. 4, pp. 357–364, 2008. View at Publisher · View at Google Scholar · View at Scopus
  12. R. Donato, “S100: a multigenic family of calcium-modulated proteins of the EF-hand type with intracellular and extracellular functional roles,” International Journal of Biochemistry and Cell Biology, vol. 33, no. 7, pp. 637–668, 2001. View at Publisher · View at Google Scholar · View at Scopus
  13. B. W. Schäfer and C. W. Heizmann, “The S100 family of EF-hand calcium-binding proteins: functions and pathology,” Trends in Biochemical Sciences, vol. 21, no. 4, pp. 134–140, 1996. View at Publisher · View at Google Scholar · View at Scopus
  14. R. L. Eckert, A. Broome, M. Ruse, N. Robinson, D. Ryan, and K. Lee, “S100 proteins in the epidermis,” Journal of Investigative Dermatology, vol. 123, no. 1, pp. 23–33, 2004. View at Publisher · View at Google Scholar · View at Scopus
  15. Z. Hua, J. Chen, B. Sun et al., “Specific expression of osteopontin and S100A6 in hepatocellular carcinoma,” Surgery, vol. 149, no. 6, pp. 783–791, 2011. View at Publisher · View at Google Scholar · View at Scopus
  16. H. Kawai, Y. Minamiya, and N. Takahashi, “Prognostic impact of S100A9 overexpression in non-small cell lung cancer,” Tumor Biology, vol. 32, no. 4, pp. 641–646, 2011. View at Publisher · View at Google Scholar · View at Scopus
  17. B. C. Yoo, Y. K. Shin, S. B. Lim, S. H. Hong, S. Y. Jeong, and J. G. Park, “Evaluation of calgranulin B in stools from the patients with colorectal cancer,” Diseases of the Colon and Rectum, vol. 51, no. 11, pp. 1703–1709, 2008. View at Publisher · View at Google Scholar · View at Scopus
  18. M. A. J. Weterman, G. M. Stoopen, G. N. P. van Muijen, J. Kuznicki, D. J. Ruiter, and H. P. J. Bloemers, “Expression of calcyclin in human melanoma cell lines correlates with metastatic behavior in nude mice,” Cancer Research, vol. 52, no. 5, pp. 1291–1296, 1992. View at Scopus
  19. R. Ciarcia, D. D'Angelo, C. Pacilio et al., “Dysregulated calcium homeostasis and oxidative stress in chronic myeloid leukemia (CML) cells,” Journal of Cellular Physiology, vol. 224, no. 2, pp. 443–453, 2010. View at Publisher · View at Google Scholar · View at Scopus
  20. K. J. Davies, “Protein damage and degradation by oxygen radicals. I. general aspects,” The Journal of Biological Chemistry, vol. 262, no. 20, pp. 9895–9901, 1987. View at Scopus
  21. I. Dalle-Donne, R. Rossi, R. Colombo, D. Giustarini, and A. Milzani, “Biomarkers of oxidative damage in human disease,” Clinical Chemistry, vol. 52, no. 4, pp. 601–623, 2006. View at Publisher · View at Google Scholar · View at Scopus
  22. L. Packer and E. Cadenas, “Oxidants and antioxidants revisited. New concepts of oxidative stress,” Free Radical Research, vol. 41, no. 9, pp. 951–952, 2007. View at Publisher · View at Google Scholar · View at Scopus
  23. R. H. Burdon, “Superoxide and hydrogen peroxide in relation to mammalian cell proliferation,” Free Radical Biology and Medicine, vol. 18, no. 4, pp. 775–794, 1995. View at Publisher · View at Google Scholar · View at Scopus
  24. H. S. Black, “The defensive role of anti-oxidants in skin carcinogenesis,” in Oxidative Stress in Dermatology, J. Fuchs and L. Packer, Eds., pp. 243–269, Marcel Dekker, New York, NY, USA, 1993.
  25. Y. Zhang, W. Zhao, H. J. Zhang, F. E. Domann, and L. W. Oberley, “Overexpression of copper zinc superoxide dismutase suppresses human glioma cell growth,” Cancer Research, vol. 62, no. 4, pp. 1205–1212, 2002. View at Scopus
  26. C. Weydert, B. Roling, J. Liu et al., “Suppression of the malignant phenotype in human pancreatic cancer cells by the overexpression of manganese superoxide dismutase,” Molecular Cancer Therapeutics, vol. 2, no. 4, pp. 361–369, 2003. View at Scopus
  27. L. Y. Chang, J. W. Slot, H. J. Geuze, and J. D. Crapo, “Molecular immunocytochemistry of the CuZn superoxide dismutase in rat hepatocytes,” Journal of Cell Biology, vol. 107, no. 6 I, pp. 2169–2179, 1988. View at Scopus
  28. H. Muramatsu, K. Kogawa, M. Tanaka et al., “Superoxide dismutase in SAS human tongue carcinoma cell line is a factor defining invasiveness and cell motility,” Cancer Research, vol. 55, no. 24, pp. 6210–6214, 1995. View at Scopus
  29. M. Tanaka, K. Kogawa, Y. Nishihori et al., “Suppression of intracellular Cu–Zn SOD results in enhanced motility and metastasis of Meth A sarcoma cells,” International Journal of Cancer, vol. 73, no. 2, pp. 187–192, 1997. View at Publisher · View at Google Scholar
  30. J. George, S. Prasad, Z. Mahmood, and Y. Shukla, “Studies on glyphosate-induced carcinogenicity in mouse skin: a proteomic approach,” Journal of Proteomics, vol. 73, no. 5, pp. 951–964, 2010. View at Publisher · View at Google Scholar · View at Scopus
  31. C. Delescluse, N. Ledirac, G. de Sousa, M. Pralavorio, P. Lesca, and R. Rahmani, “Cytotoxic effects and induction of cytochromes P450 1A1/2 by insecticides, in hepatic or epidermal cells: binding capability to the Ah receptor,” Toxicology Letters, vol. 96-97, pp. 33–39, 1998. View at Publisher · View at Google Scholar · View at Scopus
  32. E. Vega-Avila and M. K. Pugsley, “An overview of colorimetric assay methods used to assess survival or proliferation of mammalian cells,” Proceedings of the Western Pharmacology Society, vol. 54, pp. 10–14, 2011. View at Scopus
  33. A. Arora, K. Seth, N. Kalra, and Y. Shukla, “Modulation of P-glycoprotein-mediated multidrug resistance in K562 leukemic cells by indole-3-carbinol,” Toxicology and Applied Pharmacology, vol. 202, no. 3, pp. 237–243, 2005. View at Publisher · View at Google Scholar · View at Scopus
  34. L. Chen, L. Liu, and S. Huang, “Cadmium activates the mitogen-activated protein kinase (MAPK) pathway via induction of reactive oxygen species and inhibition of protein phosphatases 2A and 5,” Free Radical Biology and Medicine, vol. 45, no. 7, pp. 1035–1044, 2008. View at Publisher · View at Google Scholar · View at Scopus
  35. W. F. Heydens, C. E. Healy, K. J. Hotz et al., “Genotoxic potential of glyphosate formulations: mode-of-action investigations,” Journal of Agricultural and Food Chemistry, vol. 56, no. 4, pp. 1517–1523, 2008. View at Publisher · View at Google Scholar · View at Scopus
  36. C. Bolognesi, G. Carrasquilla, S. Volpi, K. R. Solomon, and E. J. P. Marshall, “Biomonitoring of genotoxic risk in agricultural workers from five Colombian regions: association to occupational exposure to glyphosate,” Journal of Toxicology and Environmental Health A, vol. 72, no. 15-16, pp. 986–997, 2009. View at Publisher · View at Google Scholar · View at Scopus
  37. M. Mladinic, S. Berend, A. L. Vrdoljak, N. Kopjar, B. Radic, and D. Zeljezic, “Evaluation of genome damage and its relation to oxidative stress induced by glyphosate in human lymphocytes in vitro,” Environmental and Molecular Mutagenesis, vol. 50, no. 9, pp. 800–807, 2009. View at Publisher · View at Google Scholar · View at Scopus
  38. R. Gniadecki and B. Gajkowska, “Intracellular calcium pool emptying induces DNA synthesis in HaCaT keratinocytes,” Experimental Dermatology, vol. 12, no. 4, pp. 453–459, 2003. View at Publisher · View at Google Scholar · View at Scopus
  39. B. Pajak and A. Orzechowski, “Chapter 4: regulation of Clusterin activity by calcium,” Advances in cancer research, vol. 104, pp. 33–58, 2009. View at Scopus
  40. C. Elie-Caille, C. Heu, C. Guyon, and L. Nicod, “Morphological damages of a glyphosate-treated human keratinocyte cell line revealed by a micro- to nanoscale microscopic investigation,” Cell Biology and Toxicology, vol. 26, no. 4, pp. 331–339, 2010. View at Publisher · View at Google Scholar · View at Scopus
  41. R. Das, A. Roy, N. Dutta, and H. K. Majumder, “Reactive oxygen species and imbalance of calcium homeostasis contributes to curcumin induced programmed cell death in Leishmania donovani,” Apoptosis, vol. 13, no. 7, pp. 867–882, 2008. View at Publisher · View at Google Scholar · View at Scopus
  42. X. H. Cao, S. S. Zhao, D. Y. Liu et al., “ROS-Ca2+ is associated with mitochondria permeability transition pore involved in surfactin-induced MCF-7 cells apoptosis,” Chemico-Biological Interactions, vol. 190, no. 1, pp. 16–27, 2011. View at Publisher · View at Google Scholar · View at Scopus
  43. V. Martín, F. Herrera, G. García-Santos, I. Antolín, J. Rodriguez-Blanco, and C. Rodriguez, “Signaling pathways involved in antioxidant control of glioma cell proliferation,” Free Radical Biology and Medicine, vol. 42, no. 11, pp. 1715–1722, 2007. View at Publisher · View at Google Scholar · View at Scopus
  44. M. Molinari, “Cell cycle checkpoints and their inactivation in human cancer,” Cell Proliferation, vol. 33, no. 5, pp. 261–274, 2000. View at Publisher · View at Google Scholar · View at Scopus
  45. Z. A. Stewart, M. D. Westfall, and J. A. Pietenpol, “Cell-cycle dysregulation and anticancer therapy,” Trends in Pharmacological Sciences, vol. 24, no. 3, pp. 139–145, 2003. View at Publisher · View at Google Scholar · View at Scopus
  46. P. Kowalczyk, M. C. Kowalczyk, J. J. Junco et al., “The possible separation of 12-O-tetradecanoylphorbol-13-acetate-induced skin inflammation and hyperplasia by compound A,” Molecular Carcinogenesis, vol. 52, no. 6, pp. 488–496, 2013. View at Publisher · View at Google Scholar · View at Scopus
  47. J. Schlingemann, J. Hess, G. Wrobel et al., “Profile of gene expression induced by the tumour promotor TPA in murine epithelial cells,” International Journal of Cancer, vol. 104, no. 6, pp. 699–708, 2003. View at Publisher · View at Google Scholar · View at Scopus
  48. S. Tyagi, J. George, R. Singh, K. Bhui, and Y. Shukla, “Neoplastic alterations induced in mammalian skin following mancozeb exposure using in vivo and in vitro models,” OMICS, vol. 15, no. 3, pp. 155–167, 2011. View at Publisher · View at Google Scholar · View at Scopus
  49. E. D. Emberley, L. C. Murphy, and P. H. Watson, “S100 proteins and their influence on pro-survival pathways in cancer,” Biochemistry and Cell Biology, vol. 82, no. 4, pp. 508–515, 2004. View at Publisher · View at Google Scholar · View at Scopus
  50. C. Gebhardt, J. Németh, P. Angel, and J. Hess, “S100A8 and S100A9 in inflammation and cancer,” Biochemical Pharmacology, vol. 72, no. 11, pp. 1622–1631, 2006. View at Publisher · View at Google Scholar · View at Scopus
  51. W. Leśniak, P. Ł. Słomnicki, and A. Filipek, “S100A6—new facts and features,” Biochemical and Biophysical Research Communications, vol. 390, no. 4, pp. 1087–1092, 2009. View at Publisher · View at Google Scholar
  52. M. Sastry, R. R. Ketchem, O. Crescenzi et al., “The three-dimensional structure of Ca2+-bound calcyclin: implications for Ca2+-signal transduction by S100 proteins,” Structure, vol. 6, no. 2, pp. 223–231, 1998. View at Scopus
  53. C. J. Hanson, M. D. Bootman, and H. L. Roderick, “Cell signalling: IP3 receptors channel calcium into cell death,” Current Biology, vol. 14, no. 21, pp. R933–R935, 2004. View at Publisher · View at Google Scholar · View at Scopus
  54. R. L. Patterson, D. Boehning, and S. H. Snyder, “Inositol 1,4,5-trisphosphate receptors as signal integrators,” Annual Review of Biochemistry, vol. 73, pp. 437–465, 2004. View at Publisher · View at Google Scholar · View at Scopus
  55. S. Orrenius, B. Zhivotovsky, and P. Nicotera, “Regulation of cell death: the calcium-apoptosis link,” Nature Reviews Molecular Cell Biology, vol. 4, no. 7, pp. 552–565, 2003. View at Publisher · View at Google Scholar · View at Scopus
  56. S. K. Joseph and G. Hajnóczky, “IP3 receptors in cell survival and apoptosis: Ca2+ release and beyond,” Apoptosis, vol. 12, no. 5, pp. 951–968, 2007. View at Publisher · View at Google Scholar · View at Scopus
  57. D. Boehning, R. L. Patterson, L. Sedaghat, N. O. Glebova, T. Kurosaki, and S. H. Snyder, “Cytochrome c binds to inositol (1,4,5) trisphosphate receptors, amplifying calcium-dependent apoptosis,” Nature Cell Biology, vol. 5, no. 12, pp. 1051–1061, 2003. View at Publisher · View at Google Scholar · View at Scopus
  58. R. Chen, I. Valencia, F. Zhong et al., “Bcl-2 functionally interacts with inositol 1,4,5-trisphosphate receptors to regulate calcium release from the ER in response to inositol 1,4,5-trisphosphate,” Journal of Cell Biology, vol. 166, no. 2, pp. 193–203, 2004. View at Publisher · View at Google Scholar · View at Scopus
  59. Y. Rong, A. S. Aromolaran, G. Bultynck et al., “Targeting Bcl-2-IP3 receptor interaction to reverse Bcl-2's inhibition of apoptotic calcium signals,” Molecular Cell, vol. 31, no. 2, pp. 255–265, 2008. View at Publisher · View at Google Scholar · View at Scopus
  60. C. White, C. Li, J. Yang et al., “The endoplasmic reticulum gateway to apoptosis by Bcl-XL modulation of the InsP3R,” Nature Cell Biology, vol. 7, no. 10, pp. 1021–1028, 2005. View at Publisher · View at Google Scholar · View at Scopus
  61. T. Jayaraman and A. R. Marks, “T cells deficient in inositol 1,4,5-trisphosphate receptor are resistant to apoptosis,” Molecular and Cellular Biology, vol. 17, no. 6, pp. 3005–3012, 1997. View at Scopus
  62. T. Szado, V. Vanderheyden, J. B. Parys et al., “Phosphorylation of inositol 1,4,5-trisphosphate receptors by protein kinase B/Akt inhibits Ca2+ release and apoptosis,” Proceedings of the National Academy of Sciences of the United States of America, vol. 105, no. 7, pp. 2427–2432, 2008. View at Publisher · View at Google Scholar · View at Scopus
  63. L. Scorrano, S. A. Oakes, J. T. Opferman et al., “BAX and BAK regulation of endoplasmic reticulum Ca2+: a control point for apoptosis,” Science, vol. 300, no. 5616, pp. 135–139, 2003. View at Publisher · View at Google Scholar · View at Scopus
  64. Y. Rong and C. W. Distelhorst, “Bcl-2 protein family members: versatile regulators of calcium signaling in cell survival and apoptosis,” Annual Review of Physiology, vol. 70, pp. 73–91, 2008. View at Publisher · View at Google Scholar · View at Scopus