Fluoxetine affects cytosolic cAMP, ATP, Ca2+ responses to forskolin, and survival of human ovarian granulosa tumor COV434 cells

Thi Mong Diep Nguyen; Danièle Klett; Yves Combarnous

doi:10.4196/kjpp.2021.25.3.189

Journal List > Korean J Physiol Pharmacol > v.25(3) > 1146694

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Nguyen, Klett, and Combarnous: Fluoxetine affects cytosolic cAMP, ATP, Ca2+ responses to forskolin, and survival of human ovarian granulosa tumor COV434 cells

Original Article

Korean J. Physiol. Pharmacol. 2021;25(3):189-195.

Published online: 1 May 2021

DOI: https://doi.org/10.4196/kjpp.2021.25.3.189

Fluoxetine affects cytosolic cAMP, ATP, Ca²⁺ responses to forskolin, and survival of human ovarian granulosa tumor COV434 cells

Thi Mong Diep Nguyen^1,^2,^*, Danièle Klett¹, Yves Combarnous¹

¹Physiologie de la Reproduction & des Comportements Laboratory, Centre National de la Recherche Scientifique (CNRS), Institut National de la Recherche Agronomique & Environnementale (INRAe), University of Tours, Nouzilly 37380, France

²Faculty of Natural Sciences, Quy Nhon University, Quy Nhon 820000, Vietnam

^*Correspondence Thi Mong Diep Nguyen, E-mail: nguyenthimongdiep@qnu.edu.vn

Received 5 October 2020 Revised 18 November 2020 Accepted 7 January 2021

(open-access):

This is an open-access article distributed under the terms of the Creative Commons Attribution Non-Commercial License (http://creativecommons.org/licenses/by-nc/4.0) which permits unrestricted non-commercial use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

Fluoxetine (FLX), a selective serotonin reuptake inhibitor antidepressant, exhibits various other mechanisms of action in numerous cell types and has been shown to induce cell death in cancer cells, paving the way for its potential use in cancer therapy. The aim of this study was to determine the off-target effects of the anti-depressant drug FLX, on the human ovarian granulosa tumor COV434 cells stimulated by forskolin (FSK), by measuring the real-time kinetics of intracellular cyclic AMP (cAMP), ATP level, cytoplasmic calcium ([Ca²⁺]_cyt) and survival of COV434 cells. We show that incubating COV434 cells with FLX (between 0.6 and 10 µM) induces a decrease in intracellular cAMP response to FSK, a drop in ATP content and stimulates cytoplasmic Ca²⁺ accumulation in COV434 cells. Only the highest concentrations of FLX (5–10 µM) diminished cell viability. The present report is the first to identify an action mechanism of FLX in human tumor ovarian cells COV434 cells and thus opening the way to potential use of fluoxetine as a complementary tool, in granulosa tumor treatments.

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Keywords: Cyclic AMP, Fluoxetine, Forskolin, Ovary, Tumor

INTRODUCTION

The selective serotonin reuptake inhibitor FLX ((7)-N-methyl-3-phenyl-3-(α,α,α-trifluoro-p-tolyloxy)propylamine hydrochloride) is the active molecule in Prozac, shown to be effective in the treatment of depression [1 -3]. Besides, FLX has off-target effects as it inhibits the activity of the voltage-dependent Na⁺ and K⁺ and Ca²⁺ channels at the plasma membrane [4,5] and is also distributed inside the cell, in the mitochondria (60–70%), synaptosomes, and other cellular organelles [6].

Cyclic adenosine 3’5’monophosphate (cAMP) and Ca²⁺ are two major intracellular second messengers of hormones, neuromediators, or cytokines functions. cAMP regulates many cellular responses, including cell growth and differentiation, gene transcription, and protein expression [7]. It is synthesized from ATP via the catalysis by adenylate cyclases (AC) and is inactivated by its hydrolysis into AMP catalyzed by nucleotide phosphodiesterases (PDE) [8]. It has been shown that the cAMP signaling pathway mediates many physiological processes like growth, reproduction and apoptosis [9]. The concentration of cytoplasmic calcium ion ([Ca²⁺]_cyt) also has a major role in cell proliferation, migration, gene regulation, or apoptosis [10,11]. These changes can happen through extracellular Ca²⁺ entry, or intracellular Ca²⁺ stores mobilization [11,12] or to a mitochondrial matrix Ca²⁺ overload, itself probably caused by mitochondrial membrane permeability alterations [13,14].

In previous studies, we have shown that FLX exerts an inhibitory effect on the cAMP response of mouse Leydig tumor cells (mLTC) to the gonadotropins luteinizing hormone (LH) and chorionic gonadotropin through different mechanisms [15]. In order to ascertain whether it is also the case in ovarian tumor cells, potentially sensitive to follicle-stimulating hormone (FSH), we undertook a similar study with COV434 cells [16]. COV434 cells were chosen because they derive from ovarian cells, initially sensitive to the gonadotropin FSH that is central in reproduction control. However, COV434 cells, maybe because of their tumoral status, appeared to be insensitive to FSH and we chose to stimulate them with forskolin (FSK), a direct activator of adenylate cyclase, to study their cAMP pathway. The main purpose of our study was to study the sensitivity of their cAMP pathway to FLX at low concentrations but we also followed its effects on intracytoplasmic Ca²⁺ and ATP.

Our data show for the first time that FLX promotes a dose-dependent inhibition of FSK-stimulated cAMP accumulation in COV434 cells, reminiscent to its effect on mLTC cells, in response to LH but at lower concentrations (0.6–10 µM) than in mLTC cells (12.5–100 µM) [15]. Moreover, we also show for the first time in COV434 cells that FLX provokes a dose-dependent increase in [Ca²⁺]_cytand a dose-dependent decrease in ATP level, with significant decrease on this tumor cell line viability at 5–10 µM FLX concentrations, suggesting its possible use as a complementary tool in granulosa tumor treatments.

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METHODS

Chemicals and reagents

All chemicals were purchased from Sigma-Aldrich (Saint Quentin Fallavier, France) unless otherwise noted. pGlosensor–TM-22F cyclic AMP plasmid and CellTiter-Blue Cell viability assay (G8080) were from Promega (Charbonnières-les-Bains, France), XtremeGENE HP DNA transfection reagent was from Roche (Boulogne-Billancourt, France).

Cell culture and plasmids, transfections

The COV434 cells (human ovarian granulosa tumor) were obtained from Sigma (France). Cells were expanded in supplemented DMEM medium (Gibco, Invitrogen, 10% fetal bovine serum, 50 µg/ml gentamicin, 10 units of penicillin/ml, and 10 µg/ml streptomycin). The cells were grown at 37°C and 5% CO₂ and were used between their 8th and 35th passage.

COV434 cells (about 100,000 cells per well) on a 96-well Greiner white/clear bottom plate (Dutscher, Brumath, France) were transfected with pGlosensor–TM -22F cyclic AMP plasmid using XtremeGENE HP DNA transfection reagent. Thirty minutes before transfection, DNA (100 ng plasmid per well) and XtremeGENE HP DNA transfection reagent (0.3 µl per well) were mixed with serum-free RPMI medium. This plasmid consists of the firefly luciferase sequence fused to that of the PKA cAMP-binding domain in a way that allows control of its enzymatic activity by cyclic AMP. The plates were then incubated overnight at 37°C under 5% CO₂ before use in the assays.

cAMP quantitation

Transfection supernatants were removed and replaced with medium deprived of fetal-calf serum (100 µl) and containing the luciferase substrate luciferin as well as 1 mM isobutyl-methyl-xanthine (IBMX) in order to inhibit endogenous nucleotide PDE activity. The plates were incubated for 2 h or 24 h with FLX at various concentrations in a 10 µl volume. Finally, FSK was added in a 10 µl volume in triplicate wells to reach 10 µM concentration. Kinetics of intracellular oxyluciferin luminescence were then recorded using a Polarstar Optima luminometer (BMG Labtech, Champigny-sur-Marne, France).

COV434 cells viability assessment

COV434 cells were seeded in 96-well plates at 100,000 cells/well. Two days later, the medium was replaced with serum-free medium in the absence (control) or presence of FLX (0–10 µM) for 2 h or 24 h at 37°C before the addition of 20 µl of CellTiter-Blue Reagent (Promega, Madison, WI, USA) to each well. After having incubated, changes in fluorescence were recorded with a Spectra Gemini spectrofluorimeter (Molecular Devices, Sunnyvale, CA, USA) at an excitation wavelength of 560 nm and an emission wavelength of 590 nm. The fluorescent signal from the CellTiter-Blue Reagent is proportional to the number of viable cells.

Intracellular adenosine triphosphate (ATP) concentration measurement

After the incubation of cells with or without FLX, the ATP level in cells was measured using the CellTiter-Glo 2.0 Assay (Promega). Standards were prepared from ATP standard (Promega) using serial dilutions to obtain concentrations of 1 × 10^–10, 1 × 10^–11, and 1 × 10^–12 M. The assay buffer and substrate were equilibrated to room temperature, and the buffer was transferred with the substrate. After 30 min, a 50 µl sample of this solution was added to 100 µl luciferin/luciferase reagent in 96-well white plates, and the content was mixed for 2 min and incubation was continued for 10 min at room temperature. The luminescence was read with an integration time of 1,000 ms using an Ascent Luminoskan Luminometer (Thermo-Fisher Scientific, Illkirch, France) with PBS as a blank.

Intracellular Ca²⁺ concentration measurement

The variation in cytoplasmic Ca²⁺ concentration ([Ca²⁺]_cyt) was assessed using the fluorescent Ca²⁺ indicator Fluo4-AM. COV434 cells were incubated with different FLX concentrations for 2 h before adding Fluo4-AM, and new incubation was carried out for 30 min at 37°C in the dark, before three washings with PBS. Changes in fluorescence were recorded with a Spectra Gemini spectrofluorimeter (Molecular Devices) at an excitation wavelength of 494 nm and an emission wavelength of 516 nm. Intracellular Ca²⁺ level calculations after the incubation period were based on the given dissociation constant Kd (Ca²⁺) = 345 nM of Fluo4-AM (Molecular Probes). The [Ca²⁺]_cyt was calculated using the equation [Ca²⁺]_cyt = Kd (F – F_min) / (F_max– F). Maximum fluorescence was determined using 50 µM calcium ionophore A23187 in the presence of 2 mM Ca²⁺, and minimal fluorescence was determined in the absence of Ca²⁺ and the presence of 2 mM EDTA.

Area under curve (AUC) calculations and statistical analyses

The GraphPad 5.0 (GraphPad Software, San Diego, CA, USA) was used for AUC determinations of individual kinetics. Mean, and SEM values for each triplicate AUCs were determined. The AUC ratios were used to compare cAMP response kinetics. One-way ANOVA with Dunnett’s test was also performed using this package. The level of significance was p < 0.05.

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RESULTS

Effect of fluoxetine on the intracellular cyclic AMP response to FSK

The effects of FLX on FSK-stimulated intracellular cAMP in COV434 cells were measured at FLX concentrations ranging between 0 and 10 µM. Fig. 1 shows that the FSK-stimulated cAMP-dependent oxiluciferin fluorescence kinetics are significantly decreased by FLX in dose-dependent and time-dependent manner as calculated by the AUC. Almost full inhibition was observed after a 2-h preincubation with 10 µM FLX final concentration (Fig. 1A, B) and the same was observed with only 5 µM FLX after a 24-h preincubation before FSK addition (Fig. 1C, D).

Fig. 1

Effect of fluoxetine (FLX) on intracellular cAMP response of COV434 cells to 10 µM forskolin (FSK).

Cells were treated with the indicated concentrations of fluoxetine for 2 h (A, B) or 24 h (C, D). (A, C) Real-time recording of luminescence under stimulation of COV434 cells by 10 µM FSK in the presence of fluoxetine; (B, D) Dose-dependent response to fluoxetine determined by the area under curve (AUC) of individual kinetics in (A, C). Different letters (^a–e) in each incubation time indicate significant differences between control and treatment at p < 0.05.

Effects of fluoxetine on ATP level in COV434 cells and on their viability

The ATP level in COV434 cells was measured after 2 or 24 h of incubation with various FLX concentrations using the ATP Cell-Titer-Glo Assay. Fig. 2A shows that FLX provokes a dose- and time-dependent decrease in the ATP level.

Fig. 2

Effect of fluoxetine (FLX) on ATP levels in COV434 cells and the number of viable COV434 cells.

ATP level (A) and the viability of COV434 cells (B) were measured after incubation with various concentrations of FLX for 2 h or 24 h. The experiments were repeated four times; values are mean ± SEM. Different letters (^a–e) in each incubation time indicate significant differences between control and treatment at p < 0.05.

After 2 or 24 h of incubation in the presence of FLX (0.625–10 µM) and a one-hour further incubation with CellTiter-Blue Assay, cell viability was found to be unaffected when compared to control at all concentrations, except at 10 µM for 2 h and ≥ 5 µM for 24 h (Fig. 2B).

Effects of fluoxetine on cytoplasmic Ca²⁺ in COV434 cells

The cytoplasmic free Ca²⁺ concentration ([Ca²⁺]_cyt) in intact cells, calculated before the addition of 5 mM extracellular Ca²⁺, was approximately 80 nM at 37°C. FLX at concentrations between 0.6125 and 10 µM induced a dose-dependent rapid rise of [Ca²⁺]_cyt up to a plateau at approximately 900 nM (Fig. 3A, B). Thus, the addition of FLX induced a sustained increase in [Ca²⁺]_cytwhen Ca²⁺ is present in the culture medium. In the absence of Ca²⁺ in the medium, FLX also led to an increase in [Ca²⁺]_cyt, but this increase was only transient (Fig. 3C). When Ca²⁺ was introduced in the culture medium, [Ca²⁺]_cyt was again increased (Fig. 3D).

Fig. 3

Effect of fluoxetine (FLX) on [Ca²⁺]_cyt in Fluo4-AM-loaded COV434 cells.

Cells were incubated with Fluo4-AM as described in experimental procedures. The intracellular Ca²⁺ levels were measured spectrofluorimetry using an excitation wavelength of 494 nm and an emission wavelength of 516 nm. The [Ca²⁺]_cyt measurements were made every 52 sec. (A) Baseline levels of [Ca²⁺]_cyt were monitored for 156 sec prior to adding Ca²⁺ at 2 mM final concentration, changes in [Ca²⁺]_cyt were monitored for an additional 800 sec. (B) Dose-dependent response to fluoxetine determined by the area under curve (AUC) of individual kinetics in (A). (C) Signal of Ca²⁺ responses induced by FLX (10 µM) in a Ca²⁺-free medium and Control (Ctrl) (absence of FLX). (D) Cells loaded with Fluo4-AM were incubated first with 10 µM FLX in Ca²⁺-free medium, and external Ca²⁺ was added after 1,000 sec. Asterisks in each concentration indicate significant differences between control and treatment at p < 0.05.

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DISCUSSION

We have previously documented that fluoxetine (FLX) exerts a dose-dependent and time-dependent inhibition of LH-stimulated cAMP accumulation in mouse Leydig tumoral cells. The data in the present paper demonstrate that FLX also rapidly inhibits cAMP accumulation under FSK stimulation in human ovarian tumor COV434 cells. After 24 h of incubation, 5 µM FLX almost completely abolished the FSK-stimulated cAMP accumulation response. A final 10 µM FLX concentration was enough to get the same inhibition after only 2 h of incubation. These results are very similar to those observed with FLX on the LH-dependent stimulation of cAMP accumulation in mLTC cells, suggesting a common mechanism.

In order to decipher more precisely the mechanisms of FLX inhibiting cAMP accumulation in COV434 cells, we decided to also study its effects on intracellular ATP and Ca²⁺ levels as well as on cell survival. In COV434 cells, FLX caused a dose-dependent drop in intracellular ATP concentrations after 2 and 24 h incubations but with only a marginal difference between the two incubation durations. Interestingly, there was no effect of FLX on COV434 cells survival after 2 h except a slight one at the highest dose tested. After 24 h, there was a marked effect of the highest FLX concentrations tested (5–10 µM) on cell survival.

In brief, the above data show that the drop in the cAMP response to FSK as a function of FLX concentration might largely be related to diminished ATP content and but not to diminished cell viability. This is not unexpected as ATP is the substrate for adenylate cyclase to synthesize cAMP. Many previous studies have shown that FLX indirectly affects electron transport and (F₁–F₀)-ATPase activity, and thus inhibits oxidative phosphorylation in mitochondria, leading to reduce ATP [17]. However, these effects of FLX on mitochondrial activities may result from interacting with VDAC and decreasing its conductance as a channel providing passage for Ca²⁺ [18], adenine nucleotides [19], other metabolites [20,21], as well as preventing PTP opening by preventing the release of accumulated Ca²⁺ and by swelling energized mitochondria and inhibiting release of cytochrome C from mitochondria [22].

In order to study more thoroughly the mechanism of the FLX effects on COV434 cells, we have measured the effects of 0.6125 to 10 µM FLX on [Ca²⁺]_cyt. Upon Ca²⁺ addition in the medium, there was an immediate rise in [Ca²⁺]_cyt that was proportional to FLX concentration in the medium up to a plateau at approximately 900 nM at the highest FLX concentration. In the absence of Ca²⁺ in the medium, FLX induced an immediate and rapid rise of intracellular [Ca²⁺]_cyt and a secondary [Ca²⁺]_cyt rise was observed upon addition of Ca²⁺ in the medium. These data indicate that FLX stimulates an increase in intracellular [Ca²⁺]_cyt both from intracellular stores and from outside the cell. Charles et al. [23], have shown that FLX induces an increase in [Ca²⁺]_cyt by emptying the endoplasmic reticulum (ER) through the translocon, an ER Ca²⁺ leakage structure, that it also inhibits oxygen consumption and lowers mitochondrial ATP, leading to Ca²⁺ reuptake into the ER, and that Ca²⁺ quickly accumulates in the mitochondria, leading to mitochondrial Ca²⁺ overload and cell death [23].

Our data also show that concentration-dependent FLX-induced cell death occurs at the same concentration ranges that induce [Ca²⁺]_cyt rise. Normal cell viability can be altered by either Ca²⁺-dependent or -independent mechanism [24,25]. Many reports also suggest that 10–100 µM FLX induces cell death in tumor cell types such as colon cancer cells [26], Burkitt’s lymphoma cells [27], and ovarian carcinoma cells [28]. Our data also show that FLX induces cell death in COV434 cells, but at lower concentrations (5–10 µM) than in those cells. This cytotoxicity could be caused by mitochondrial Ca²⁺ overload, as it has already been shown in glioma cells [29]. At moderate concentration, mitochondrial Ca²⁺ supports ATP production by stimulating mitochondrial metabolic enzymes such as FAD-glycerol phosphate dehydrogenase, pyruvate dehydrogenase phosphatase, NAD-isocitrate dehydrogenase, oxoglutarate dehydrogenase, F₁–F₀ ATP synthase, cytochrome C oxidase [30]. But excess Ca²⁺ in the mitochondria leads to activation of both mitochondria-specific sodium/calcium exchanger (NCLX) and permeability transition pore (PTP) [31,32]. Such prolonged mitochondrial calcium permeability might end up in either apoptosis or necrosis, depending on the availability of ATP since previous works reported that weakly damaged mitochondria still contain enough ATP to trigger apoptosis, whereas more severely damaged mitochondria promote cell necrosis [33 -36].

Collectively, the results show that, via direct and/or indirect mechanisms, fluoxetine induced 1) a decreased cAMP response to FSK, 2) a decreased intracellular ATP content, 3) an increased [Ca²⁺]_cyt concentration and 4) a decreased cell viability (only at the highest FLX concentrations tested [5–10 µM], but not at the lowest concentrations [0.6–2.5 µM] already affecting the cAMP, ATP and Ca²⁺ responses). This last effect favors the use of the anti-depressant drug fluoxetine as a complementary tool, in granulosa tumor treatments, as already proposed for other cancer cell types.

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ACKNOWLEDGEMENTS

We are indebted to Prof. Virginie Maillard (Université de Tours, INRAe, PRC, Nouzilly) for her kind gift of COV434 cells, and fruitful discussions.

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Notes

Author contributions: T.M.D.N. and Y.C. designed the protocol of the study. T.M.D.N. and D.K. performed the experiments. T.M.D.N. wrote the manuscript. T.M.D.N. and Y.C. edited the manuscript.

CONFLICTS OF INTEREST

The authors declare no conflicts of interest.

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REFERENCES

1. Wong DT, Bymaster FP, Engleman EA. 1995; Prozac (fluoxetine, Lilly 110140), the first selective serotonin uptake inhibitor and an antidepressant drug: twenty years since its first publication. Life Sci. 57:411–441. DOI: 10.1016/0024-3205(95)00209-O. PMID: 7623609.

2. Stark P, Fuller RW, Wong DT. 1985; The pharmacologic profile of fluoxetine. J Clin Psychiatry. 46(3 Pt 2):7–13. PMID: 3871767.

3. Fuller RW, Wong DT, Robertson DW. 1991; Fluoxetine, a selective inhibitor of serotonin uptake. Med Res Rev. 11:17–34. DOI: 10.1002/med.2610110103. PMID: 1994152.

4. Pancrazio JJ, Kamatchi GL, Roscoe AK, Lynch C 3rd. 1998; Inhibition of neuronal Na+ channels by antidepressant drugs. J Pharmacol Exp Ther. 284:208–214. PMID: 9435180.

5. Deák F, Lasztóczi B, Pacher P, Petheö GL, Kecskeméti V, Spät A. 2000; Inhibition of voltage-gated calcium channels by fluoxetine in rat hippocampal pyramidal cells. Neuropharmacology. 39:1029–1036. DOI: 10.1016/S0028-3908(99)00206-3. PMID: 10727713.

6. Mukherjee J, Das MK, Yang ZY, Lew R. 1998; Evaluation of the binding of the radiolabeled antidepressant drug, 18F-fluoxetine in the rodent brain: an in vitro and in vivo study. Nucl Med Biol. 25:605–610. DOI: 10.1016/S0969-8051(98)00043-2. PMID: 9804041.

7. Francis SH, Corbin JD. 1994; Structure and function of cyclic nucleotide-dependent protein kinases. Annu Rev Physiol. 56:237–272. DOI: 10.1146/annurev.ph.56.030194.001321. PMID: 8010741.

8. Maurice DH, Palmer D, Tilley DG, Dunkerley HA, Netherton SJ, Raymond DR, Elbatarny HS, Jimmo SL. 2003; Cyclic nucleotide phosphodiesterase activity, expression, and targeting in cells of the cardiovascular system. Mol Pharmacol. 64:533–546. DOI: 10.1124/mol.64.3.533. PMID: 12920188.

9. Jin L, Hill KK, Filak H, Mogan J, Knowles H, Zhang B, Perraud AL, Cambier JC, Lenz LL. 2011; MPYS is required for IFN response factor 3 activation and type I IFN production in the response of cultured phagocytes to bacterial second messengers cyclic-di-AMP and cyclic-di-GMP. J Immunol. 187:2595–2601. DOI: 10.4049/jimmunol.1100088. PMID: 21813776. PMCID: PMC3159690.

10. Berridge MJ, Bootman MD, Roderick HL. 2003; Calcium signalling: dynamics, homeostasis and remodelling. Nat Rev Mol Cell Biol. 4:517–529. DOI: 10.1038/nrm1155. PMID: 12838335.

11. Berridge MJ, Lipp P, Bootman MD. 2000; The versatility and universality of calcium signalling. Nat Rev Mol Cell Biol. 1:11–21. DOI: 10.1038/35036035. PMID: 11413485.

12. Carafoli E, Santella L, Branca D, Brini M. 2001; Generation, control, and processing of cellular calcium signals. Crit Rev Biochem Mol Biol. 36:107–260. DOI: 10.1080/20014091074183. PMID: 11370791.

13. Duchen MR. 1999; Contributions of mitochondria to animal physiology: from homeostatic sensor to calcium signalling and cell death. J Physiol. 516(Pt 1):1–17. DOI: 10.1111/j.1469-7793.1999.001aa.x. PMID: 10066918. PMCID: PMC2269224.

14. Duchen MR. 2000; Mitochondria and calcium: from cell signalling to cell death. J Physiol. 529(Pt 1):57–68. DOI: 10.1111/j.1469-7793.2000.00057.x. PMID: 11080251. PMCID: PMC2270168.

15. Nguyen TMD, Klett D, Filliatreau L, Combarnous Y. 2019; Inhibition by fluoxetine of LH-stimulated cyclic AMP synthesis in tumor Leydig cells partly involves AMPK activation. PLoS One. 14:e0217519. DOI: 10.1371/journal.pone.0217519. PMID: 31163038. PMCID: PMC6548379.

16. Zhang H, Vollmer M, De Geyter M, Litzistorf Y, Ladewig A, Dürrenberger M, Guggenheim R, Miny P, Holzgreve W, De Geyter C. 2000; Characterization of an immortalized human granulosa cell line (COV434). Mol Hum Reprod. 6:146–153. DOI: 10.1093/molehr/6.2.146. PMID: 10655456.

17. Curti C, Mingatto FE, Polizello AC, Galastri LO, Uyemura SA, Santos AC. 1999; Fluoxetine interacts with the lipid bilayer of the inner membrane in isolated rat brain mitochondria, inhibiting electron transport and F1F0-ATPase activity. Mol Cell Biochem. 199:103–109. DOI: 10.1023/A:1006912010550. PMID: 10544958.

18. Gincel D, Zaid H, Shoshan-Barmatz V. 2001; Calcium binding and translocation by the voltage-dependent anion channel: a possible regulatory mechanism in mitochondrial function. Biochem J. 358(Pt 1):147–155. DOI: 10.1042/bj3580147. PMCID: PMC1222042. PMID: 11485562.

19. Rostovtseva T, Colombini M. 1997; VDAC channels mediate and gate the flow of ATP: implications for the regulation of mitochondrial function. Biophys J. 72:1954–1962. DOI: 10.1016/S0006-3495(97)78841-6. PMID: 9129800. PMCID: PMC1184392.

20. Hodge T, Colombini M. 1997; Regulation of metabolite flux through voltage-gating of VDAC channels. J Membr Biol. 157:271–279. DOI: 10.1007/s002329900235. PMID: 9178614.

21. Shoshan-Barmatz V, Gincel D. 2003; The voltage-dependent anion channel: characterization, modulation, and role in mitochondrial function in cell life and death. Cell Biochem Biophys. 39:279–292. DOI: 10.1385/CBB:39:3:279. PMID: 14716081.

22. Nahon E, Israelson A, Abu-Hamad S, Varda SB. 2005; Fluoxetine (Prozac) interaction with the mitochondrial voltage-dependent anion channel and protection against apoptotic cell death. FEBS Lett. 579:5105–5110. DOI: 10.1016/j.febslet.2005.08.020. PMID: 16139271.

23. Charles E, Hammadi M, Kischel P, Delcroix V, Demaurex N, Castelbou C, Vacher AM, Devin A, Ducret T, Nunes P, Vacher P. 2017; The antidepressant fluoxetine induces necrosis by energy depletion and mitochondrial calcium overload. Oncotarget. 8:3181–3196. DOI: 10.18632/oncotarget.13689. PMID: 27911858. PMCID: PMC5356874.

24. Costa-Junior HM, Mendes AN, Davis GH, da Cruz CM, Ventura AL, Serezani CH, Faccioli LH, Nomizo A, Freire-de-Lima CG, Bisaggio Rda C, Persechini PM. 2009; ATP-induced apoptosis involves a Ca₂₊-independent phospholipase A2 and 5-lipoxygenase in macrophages. Prostaglandins Other Lipid Mediat. 88:51–61. DOI: 10.1016/j.prostaglandins.2008.09.004. PMID: 18984060.

25. Sakanashi Y, Oyama TM, Matsuo Y, Oyama TB, Nishimura Y, Ishida S, Imai S, Okano Y, Oyama Y. 2009; Zn₂₊, derived from cell preparation, partly attenuates Ca₂₊-dependent cell death induced by A23187, calcium ionophore, in rat thymocytes. Toxicol In Vitro. 23:338–345. DOI: 10.1016/j.tiv.2008.12.006. PMID: 19124067.

26. Kannen V, Hintzsche H, Zanette DL, Silva WA Jr, Garcia SB, Waaga-Gasser AM, Stopper H. 2012; Antiproliferative effects of fluoxetine on colon cancer cells and in a colonic carcinogen mouse model. PLoS One. 7:e50043. DOI: 10.1371/journal.pone.0050043. PMID: 23209640. PMCID: PMC3507893.

27. Cloonan SM, Williams DC. 2011; The antidepressants maprotiline and fluoxetine induce Type II autophagic cell death in drug-resistant Burkitt's lymphoma. Int J Cancer. 128:1712–1723. DOI: 10.1002/ijc.25477. PMID: 20503272.

28. Lee CS, Kim YJ, Jang ER, Kim W, Myung SC. 2010; Fluoxetine induces apoptosis in ovarian carcinoma cell line OVCAR-3 through reactive oxygen species-dependent activation of nuclear factor-kappaB. Basic Clin Pharmacol Toxicol. 106:446–453. DOI: 10.1111/j.1742-7843.2009.00509.x. PMID: 20050848.

29. Brambilla P, Cipriani A, Hotopf M, Barbui C. 2005; Side-effect profile of fluoxetine in comparison with other SSRIs, tricyclic and newer antidepressants: a meta-analysis of clinical trial data. Pharmacopsychiatry. 38:69–77. DOI: 10.1055/s-2005-837806. PMID: 15744630.

30. Tarasov AI, Griffiths EJ, Rutter GA. 2012; Regulation of ATP production by mitochondrial Ca₂₊. Cell Calcium. 52:28–35. DOI: 10.1016/j.ceca.2012.03.003. PMID: 22502861. PMCID: PMC3396849.

31. Rizzuto R, Marchi S, Bonora M, Aguiari P, Bononi A, De Stefani D, Giorgi C, Leo S, Rimessi A, Siviero R, Zecchini E, Pinton P. 2009; Ca₂₊ transfer from the ER to mitochondria: when, how and why. Biochim Biophys Acta. 1787:1342–1351. DOI: 10.1016/j.bbabio.2009.03.015. PMID: 19341702. PMCID: PMC2730423.

32. Spät A, Szanda G, Csordás G, Hajnóczky G. 2008; High- and low-calcium-dependent mechanisms of mitochondrial calcium signalling. Cell Calcium. 44:51–63. DOI: 10.1016/j.ceca.2007.11.015. PMID: 18242694. PMCID: PMC2662195.

33. Rasola A, Bernardi P. 2011; Mitochondrial permeability transition in Ca₂₊-dependent apoptosis and necrosis. Cell Calcium. 50:222–233. DOI: 10.1016/j.ceca.2011.04.007. PMID: 21601280.

34. Rasola A, Sciacovelli M, Pantic B, Bernardi P. 2010; Signal transduction to the permeability transition pore. FEBS Lett. 584:1989–1996. DOI: 10.1016/j.febslet.2010.02.022. PMID: 20153328. PMCID: PMC2866765.

35. Leist M, Single B, Castoldi AF, Kühnle S, Nicotera P. 1997; Intracellular adenosine triphosphate (ATP) concentration: a switch in the decision between apoptosis and necrosis. J Exp Med. 185:1481–1486. DOI: 10.1084/jem.185.8.1481. PMID: 9126928. PMCID: PMC2196283.

36. Bernardi P, Rasola A. 2007; Calcium and cell death: the mitochondrial connection. Subcell Biochem. 45:481–506. DOI: 10.1007/978-1-4020-6191-2_18. PMID: 18193649.

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