| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
Department of Physiology and Biophysics (T.D., J.A.A., K.H.H., D.B.H.), University of Illinois at Chicago, Chicago, Illinois 60612-7342; and Department of Urology (T.D.), University Hospital of the Justus-Liebig-University, 35392 Giessen, Germany
Address all correspondence and requests for reprints to: Dale Buchanan Hales, Ph.D., Department of Physiology and Biophysics, University of Illinois at Chicago, 835 South Wolcott Avenue, Chicago, Illinois 60612-7342. E-mail: dbhale{at}uic.edu.
 |
Abstract |
|---|
 Top Abstract IntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
m). ROS caused a significant dissipation of m and time-dependent loss of tetramethylrhodamine ethyl ester fluorescence. The inhibitory effects of H2O2 were transient. There was no evidence for ROS-induced cell death, and following H2O2 removal in the presence of continuous treatment with 8-bromo-cAMP, StAR protein levels and progesterone production were restored. In addition, there was no loss of cell viability following treatment with H2O2 or xanthine/xanthine oxidase as determined by trypan blue exclusion. H2O2 did not cause a significant decrease in total cellular ATP levels. These data indicate that oxidative stress-mediated perturbation of the mitochondria and dissipation of m results in the inhibition of StAR protein expression and its import, processing, and cholesterol transfer activity. These findings confirm earlier studies demonstrating the requirement for maintenance of an intact m for StAR protein function in cholesterol transport. The significant reduction in the 32- to 30-kDa mature forms of StAR, cessation of cholesterol transport, and loss of m are consistent with mitochondrial perturbation because of oxidative stress. This mechanism likely contributes to a host of pathophysiological events evident in testicular disorders such as infection, reperfusion injury, aging, cryptorchidism, and varicocele. |
Introduction |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
There have been relatively few studies on the effects of ROS on steroidogenesis. ROS has been implicated in the ovary in the process of luteolysis (21, 22, 23), and earlier studies indicated that ROS blocks the hormone-sensitive cholesterol transfer step (22). ROS have also been shown to inhibit steroidogenesis in MA-10 tumor Leydig cells, also at the level of cholesterol transfer (24). ROS have also been suggested to be important to the senescence of Leydig cell function during aging (25, 26, 27).
Oxidative damage is a consequence of excessive oxidative stress, insufficient antioxidant potential, or a combination of both. Oxidative damage induced by ROS is implicated as an important contributing factor in the pathogenesis of more than 100 conditions (2). ROS include oxygen radicals such as superoxide anion and hydroxyl radical, and reactive oxygen and nitrogen species such as hydrogen peroxide (H2O2), nitric oxide, and peroxynitrite anion, which are not radicals in nature but are capable of radical formation in cellular environments. ROS cause tissue damage by a variety of mechanisms including DNA damage, lipid peroxidation, protein oxidation, depletion of cellular thiols, and activation of proinflammatory cytokine release. ROS have short half-lives; they inflict damage by initiating free radical chain reactions. Several cellular antioxidant systems are present to help protect against free radical damage. These antioxidant systems include antioxidant molecules such as 
-tocopherol, ascorbic acid, and glutathione and antioxidant enzymes such as glutathione peroxidase and superoxide dismutase. When the levels of ROS exceed the cellular antioxidant capacity, cells are subjected to oxidative stress, and oxidative damage occurs.
Mitochondria are an important cellular source of ROS and are very susceptible to oxidative damage. Oxidative damage to mitochondria is considered to be central to cellular senescence associated with aging and a host of other pathologies (4). Recently much attention has been paid to mitochondria because mutations of mitochondrial DNA are the basis of certain diseases, and perturbation of mitochondria is important to mechanisms of cell death.
Another significant role for mitochondria is as a key control point for the regulation of steroid hormone biosynthesis. The first and rate-limiting step in the biosynthesis of steroid hormones in the adrenals and gonads is the transfer of cholesterol across the inner mitochondrial space from the outer mitochondrial membrane to the inner mitochondrial membrane, a process now known to depend on the action of the steroidogenic acute regulatory protein (StAR) (28, 29). Testosterone production by Leydig cells is primarily under the control of LH, which acts via its intracellular second messenger cAMP to regulate testosterone production acutely at the level of cholesterol transport into the mitochondria via the action of StAR and chronically at the level of the steroidogenic enzyme gene transcription.
To analyze the effects of ROS on steroidogenesis, we examined the effects of H2O2 on progesterone production, and steroidogenic enzyme and StAR protein expression in MA-10 tumor Leydig cells. MA-10 cells are a convenient model to study the acute regulation of steroidogenesis because they are LH/human chorionic gonadotropin and cAMP responsive and express StAR, P450 side-chain cleavage enzyme (P450scc), and 3ß-hydroxysteroid dehydrogenase. MA-10 cells do not express P450c17 or produce testosterone to a significant degree but instead produce primarily progesterone. The purpose of this study was to examine the effects of ROS on steroidogenesis in MA-10 cells and determine the extent to which MA-10 cell mitochondria are sensitive to oxidative stress.
|
Materials and Methods |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
32P]Deoxyguanidine triphospate was from ICN Biochemicals (Irvine, CA). Enhanced chemiluminescence Western blot detection kit was from Amersham Pharmacia Biotech (Piscataway, NJ). Tetramethylrhodamine ethyl ester dye (TMRE) was from Molecular Probes, Inc. (Eugene, OR). Xanthine and xanthine oxidase were from Calbiochem (San Diego, CA). ATP bioluminescent assay kit was from Sigma. Mouse StAR cDNA and CMV-StAR were a generous gift from Douglas Stocco (Lubbock, TX).
MA-10 cell culture and treatments
MA-10 cells derived from a transplantable Leydig cell tumor in mice were a kind gift from Dr. Mario Ascoli (University of Iowa College of Medicine, Iowa City, IA) and were maintained as described previously (30). MA-10 cells were cultured in Waymouth’s complete medium MB752/1 (Invitrogen) containing 20 mM HEPES, 1.2 g/liter sodium bicarbonate, 15% heat-inactivated donor herd horse serum, 100 IU/ml penicillin, and 100 µg/ml streptomycin. MA-10 cells were grown in culture to approximately 75% confluency and were preincubated in serum-free media (SFM) for 1 h. Cells were then treated for 3 h in Waymouth’s SFM that contained 1 mM 8-Br-cAMP or cAMP plus increasing concentrations of H2O2 (10–1000 µM). A 3% stock solution of H2O2 was used, and appropriate volumes were added to Waymouth’s SFM just before cell treatments. Before treatment with xanthine oxidase, cells were preincubated with serum-free RPMI media for 1 h. Cells were then treated for 3 h in RPMI SFM that contained 1 mM 8-Br-cAMP or cAMP plus 100 µM xanthine plus increasing milliunit quantities of xanthine oxidase (1–100 mU). One milliunit xanthine oxidase will covert 1 µmol xanthine to uric acid per minute, yielding superoxide anion as a by-product. Cells were incubated at 37 C in 5% CO2 in a humidified incubator.
Northern blotting and hybridization
Extraction and analysis of total RNA was performed after lysis of cells with a guanidine-isothiocyanate-based lysis buffer followed by phenol extractions under acidic conditions and isopropanol precipitation of nucleic acids (APGC method) as described previously (31, 32, 33). Ten micrograms total RNA from each sample were analyzed. Agarose gel electrophoresis of RNA and Northern blotting to nitrocellulose paper (Millipore Corp., Bedford, MA) membranes was performed as described previously (33, 34). Northern hybridization was performed by use of 32P-labled random primed cDNA probes specific for StAR and cyclophilin (35, 36, 37, 38). Hybridization signal from the radioactively labeled Northern blots were obtained after exposure to a phosphor screen for 24 h. Hybridization signals were quantified by phosphorimaging (Storm 860, Molecular Dynamics, Inc., Sunnyvale, CA) and computer software (Image QuaNT, Molecular Dynamics, Inc.). Expression data for mRNA are expressed as integrated OD (IOD). Expression of StAR mRNA IOD has been normalized to the expression of the constitutively expressed gene cyclophilin.
Western analysis and immunodetection of proteins
After treatments, total cellular protein was obtained by placing cells in lysis buffer (PBS/0.1% SDS) followed by brief sonication (ultrasonic processor GE 50 T (Sonics, Newtown, CT), 50% power for 
2 sec). Protein concentrations were determined by microBCA protein assay (Pierce Chemical Co., Rockford, IL). Thirty micrograms total cellular protein were separated by SDS-PAGE using 10% acrylamide/SDS separating gels and transferred to nitrocellulose paper membranes as described previously (33, 39). The preparation of the polyclonal antiserum to StAR and P450scc has been described previously (40, 41). Detection of bound antibody on the blot was assessed with a horseradish peroxidase-conjugated, goat antirabbit IgG antibody (Sigma) visualized by chemiluminescent detection (ECL Western blot detection kit, Amersham Pharmacia Biotech), and quantitated after densitometry (personal densitometer, Molecular Dynamics, Inc.) using Imagequant software (Molecular Dynamics, Inc.). Expression data for protein are expressed as IOD.
Progesterone RIA
After respective cell treatments, culture media were removed and stored at -20 C until later analysis. Before assaying, culture media were boiled for 5 min and centrifuged at 2000 x g for 20 min at 4 C. Concentrations of progesterone in the media samples were determined using Coat-a-Count RIA kits (Diagnostic Products, Los Angeles, CA). Progesterone concentration in each sample was measured in duplicate. To control for variability in cell number in each culture, progesterone concentrations were normalized to protein concentrations for each sample (nanograms per milligram protein).
Cell viability assay
Cell viability was assessed by trypan blue exclusion, according to the manufacturer’s instructions. Briefly, cells were treated as described under MA-10 cell culture and treatments and in figure legends. After respective treatments, cells were trypsinized for 1 min at room temperature and then resuspended in 1x PBS. Equal volumes of resuspended cells and 0.4% trypan blue (Sigma) were combined, incubated at room temperature for 10 min, and counted using a standard hemocytometer (Fisher Scientific, Itasca, IL). Viable cells (unstained) and nonviable cells (stained) were counted, and the percent cell viability was calculated as follows: [% cell viability = total viable cells (unstained)/total cells (stained and unstained) x 100]. The viability assay was repeated for each treatment group, and the data are represented as mean ± SEM for three independent experiments.
Measurement of cellular ATP
After treatments, cells were briefly washed with cold PBS. Cells were then incubated for 15 min in a lysis/precipitation solution of 3% trichloroacetic acid and 2 mM EDTA. Cells were transferred to fresh tubes and subjected to brief sonication (ultrasonic processor GE 50 T, 50% power for approximately 2 sec, four times). Lysates were centrifuged at 3000 x g for 20 min at 4 C, and the supernatant containing total cellular ATP was collected. The supernatants containing ATP were adjusted to a pH of 7.8. Protein lysis buffer (PBS/0.1% SDS) was added to the pellet to obtain protein lysates for each sample. The lysates were briefly sonicated and protein concentrations were determined by microBCA protein assay (Pierce Chemical Co.). ATP was assayed using the ATP bioluminescent assay kit (Sigma), according to the manufacturer’s instructions. Light intensity of the sample was measured using a luminometer (Lumat 9506, EG&G Berthold, Alliquippa, PA). Standard concentrations of ATP (1–500 pmol) were prepared and a standard curve was generated. ATP concentrations in each sample were determined by linear regression analysis using Instat, version 3.0, software package for statistical data analysis (GraphPad Software, Inc., San Diego, CA). To control for variability in original cell number, ATP concentrations were normalized to protein concentrations for each sample and expressed as pmol/µg protein.
Assessment of the mitochondrial membrane potential (m)
MA-10 cells were grown on poly-L-lysine-coated glass coverslips (Fisher Scientific, Fair Lawn, NJ) and prestained with 40 nM TMRE (Molecular Probes, Inc.) for 10 min at 37 C. Cells were then transferred to a temperature-controlled microscope stage and analyzed using time-lapse video fluorescent microscopy. A polarized, intact mitochondrial potential is necessary for the uptake and accumulation of TMRE dye in mitochondria. Thus, analysis of TMRE fluorescence by microscopy allowed the semiquantitative assessment of the m as described (42). Fluorescence of the dye in Leydig cell mitochondria was visualized before treatment with H2O2. Cells were treated for 1 h with 250 µM H2O2 in SFM. At time 0 min, H2O2 was added to the cells, which were subsequently examined for 1 h using time-lapse video fluorescent microscopy. MA-10 cells in SFM alone were also examined to control for photo-bleaching artifacts. Fluorescent images were obtained using an inverted microscope equipped for fluorescent microscopy (Eclipse TE 300, 547 nm wavelength excitation, 579 nm emission, Nikon, via high pressure Xenon XBO 75 W lamp, Nikon); a digital camera (RTE/CCD-1300 Y/HS, Roper Scientific, Trenton, NJ; MicroMAX camera controller, Princeton Instruments, Trenton, NJ; 
10–2 shutter, Sutter Instruments Co., Navato, CA), and image-processing software (IPLab, Scanalytics Inc., Fairfax, VA).
Statistical analysis
Data were presented as means ± SEM of three or more independent experiments. For group comparisons, one-way ANOVA followed by Student-Newman-Keuls multiple-range tests were performed using the Instat, version 3.0, software package for statistical data analysis (GraphPad Software, Inc.). Differences are considered significant at P < 0.05.
|
Results |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
). Treatment of 8-Br-cAMP-stimulated MA-10 cells with H2O2 caused a dose-dependent decrease in progesterone production. Treatment of MA-10 cells with 100, 250, and 500 µM H2O2 caused significant decrease in cAMP-stimulated progesterone production, compared with cells treated with cAMP alone, by 44%, 68%, and 71%, respectively, to 294.3 ± 54, 169.0 ± 42, and 151.3 ± 21 ng/mg protein (n = 4, P < 0.05 for all groups).
|
). Exposure of MA-10 cells to H2O2 caused a significant decrease in cAMP-stimulated StAR protein expression. StAR protein was virtually undetectable in MA-10 cells from control cultures. Treatment with 1 mM 8-Br-cAMP for 3 h results in a significant 50-fold increase in StAR protein levels. Treatment of cAMP-stimulated MA-10 cells with H2O2 caused a dose-dependent decrease in StAR protein. Treatment of MA-10 cells with 100, 250, and 500 µM H2O2 reduced 30-/32-kDa StAR protein by 22%, 89%, and 100%, respectively, compared with cells treated with cAMP alone. Only the decreases observed with 250 and 500 µM H2O2 were significant (P < 0.05, n = 3). Although H2O2 caused a significant decrease in 30/32 kDa StAR, the 37-kDa precursor form of StAR did not decrease appreciably, suggesting that the intramitochondrial mature forms were affected to a greater extent (Fig. 2). In contrast, treatment of MA-10 cells with 1 mM 8-Br-cAMP or cAMP plus increasing concentrations of H2O2 for 3 h had no effect on P450scc protein levels (Fig. 2B).
|
). There was no difference observed in the relative expression levels of the three StAR transcripts (3.4, 2.9, and 1.9 kb). Data are presented as the ratio of the 3.4-kb StAR transcript to cyclophilin mRNA. Treatment with 1 mM 8-Br-cAMP for 3 h results in a significant 65-fold increase in StAR mRNA. In marked contrast to the effects of H2O2 on StAR protein levels, treatment of cAMP-stimulated MA-10 cells with H2O2 had no effect on StAR mRNA levels. Only treatment of MA-10 cells with cAMP plus 1000 µM H2O2 significantly reduced StAR transcript levels by 97%, compared with cells treated with cAMP alone. It is apparent that the RNA isolated from cells exposed to 1000 µM H2O2 was degraded by this concentration of H2O2 as indicated by the appearance of cyclophilin and StAR mRNA transcripts. These data indicate that StAR protein, but not mRNA, is decreased during oxidative stress, suggesting that ROS acts posttranscriptionally to inhibit StAR protein expression.
|
). Compared with untreated controls, cAMP treatment for 3 h resulted in a significant increase in 30/32 kDa StAR protein of greater than 50-fold, similar to the results shown in Fig. 2
. Treatment of cells with cAMP plus H2O2 for 3 h caused a significant decrease in StAR protein levels by 70% (P < 0.5, n = 3). Three hours after removal of H2O2 with continued treatment with cAMP alone, StAR protein levels recovered by 37%, compared with cells treated with cAMP plus H2O2 for 3 h (P < 0.05, n = 3). Progesterone concentrations were analyzed, and there was a parallel recovery of progesterone production (data not shown). When cells were exposed to H2O2 continuously for 6 h in the presence of cAMP, StAR protein levels also began to return to the level of StAR protein in cultures treated continuously with cAMP alone (data not shown).
|
). Treatment with 10, 50, and 100 mU xanthine oxidase, in the presence of 100 µM xanthine, resulted in a 29%, 31%, and 79% decrease in progesterone production, respectively.
|
, StAR protein was quantitated in cell preparations. The mature, intramitochondrial forms of StAR protein (30/32 kDa) decreased in a similar manner to changes in progesterone from the same cultures (Fig. 6). Exposure to 10, 50, and 100 mU xanthine oxidase, in the presence of 100 µM xanthine, resulted in a decrease in 30/32 kDa StAR protein by 87, 90, and 99%, respectively. In contrast, the 37-kDa extramitochondrial precursor form of StAR did not decrease as a result of xanthine oxidase treatment but was significantly increased relative to the intramitochondrial 30/32-kDa forms of StAR. As shown in Fig. 6B, treatment with 10, 50, and 100 mU xanthine oxidase, in the presence of 100 µM xanthine, resulted in a change in the 37-kDa form of StAR of 120%, 210%, and 55%, relative to cells treated with cAMP alone. When the ratio of 37 to 30/32 kDa StAR is plotted (Fig. 6C), the increase in 37 kDa relative to 30/32 kDa, as a result of exposure to xanthine oxidase, is more apparent: 10, 50, and 100 mU xanthine oxidase result in an increase in 37 to 30/32 kDa StAR of 13-, 16-, and 111-fold, in xanthine oxidase-treated cells, compared with cells treated with cAMP only. The sizes of the 37-, 32-, and 30-kDa forms of StAR were deduced from molecular mass markers and confirmed by comparison to 35S-methione labeling COS-7 cells that were transfected with CMV-StAR expression vector, immunoprecipitating overexpressed StAR protein, and subjecting it to SDS-PAGE analysis in parallel to gels used for Western blot analysis (data not shown; see Ref. 40).
|
, exposure to any of the treatments did not alter the viability of MA-10 cells. The percent of viable cells ± SEM was similar in control and cAMP- and ROS-treated cells (control: 94.8% ± 1.2%; cAMP: 91.4% ± 1.3%; cAMP+250 µM H2O2: 92.2% ± 1.3%; cAMP+10 mU XanOx: 89.8% ± 0.5%; Fig. 7).
|
). MA-10 cells were treated with control media or media that contained 1 mM 8-Br-cAMP, cAMP plus 250 µM H2O2, or cAMP plus xanthine (100 µM) and xanthine oxidase 10 mU. ATP was determined in cell lysates by bioluminescence assay as described in Materials and Methods, and data normalized to protein concentrations for each sample. Treatment of the cells with cAMP alone or cAMP plus xanthine/xanthine oxidase resulted in significant decrease in cellular ATP levels, compared with control (n = 3, P < 0.05). Control and cAMP- and cAMP plus xanthine/xanthine oxidase-treated cells had 34.9 ± 4.0, 21.8 ± 2.1, and 16.1 ± 2.8 pmol ATP/µg protein ± SEM, respectively. In cells exposed to cAMP plus H2O2, there was 28.7 ± 6.3 pmol ATP/µg protein.
|
mm were assessed by fluorescence microscopy using the lipophilic cationic dye TMRE. Lipophilic fluorochrome cations such as TMRE accumulate in the mitochondrial matrix, driven by the electrochemical gradient following the Nernst equation, and thus are useful to measure changes in m (43). MA-10 cells were grown on poly-L-lysine-coated coverslips, and then were preincubated with 40 nM TMRE for 30 min at 37 C. Cells were transferred to the temperature-controlled stage of a microscope equipped with epi-fluorescence. At time 0, 250 µM H2O2 were added to the cells and images of the cells were captured for 300 msec every 5 min for 1 h and recorded by time-lapse video capture. Select frames are shown from images captured at 0, 25, 50, 55, and 60 min. The cluster of cells shown in Fig. 9 reveal intense punctuate mitochondrial fluorescence that does not appreciably decrease for the first 25 min following addition of H2O2. Starting at 50 min post addition of H2O2, there is a rapid and extensive loss of mitochondrial fluorescence indicating that by 60 min, m has been completely dissipated. In control experiments, cell were labeled with TMRE and subjected to video capture time-lapse fluorescent microscopy without the addition of H2O2. There was no loss of fluorescence signal because of the effects of photobleaching (not shown). Mitochondrial potentials of MA-10 cells were markedly decreased over a similar time course with 100 µM H2O2. Treatment with other more lipophilic H2O2 derivatives such as t-butyl-H2O2 and cumene-H2O2 at concentrations of 50–100 µM resulted in an even more severe disruption of m (not shown).
|
|
Discussion |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
m. These data suggest that StAR protein expression and function depend on an intact m, and perturbation of the mitochondria causes a block to StAR protein expression. The 37-kDa precursor of StAR remains at a constant level during incubation with xanthine oxidase and its substrate xanthine, but the intramitochondrial 32- and 30-kDa mature forms of StAR decrease, suggesting that StAR protein expression is blocked in part at the level of mitochondrial import and processing. Previous studies of the effects of oxidative stress on steroidogenesis predicted that the main effect of ROS on steroidogenic cells is the inhibition of StAR protein function. At the time Behrman and Aten (22) and Stocco et al. (24) assessed the effects of H2O2 on steroidogenesis, the molecular identity of StAR had not yet been defined. However, in these earlier studies, the first hormonally regulated step in steroid biosynthesis, the transfer of cholesterol to the inner mitochondrial membrane, was shown to be the step in which ROS primarily exerted its effect. The studies reported herein confirm and extend these earlier observations and demonstrate that the inhibition of StAR protein by ROS is a major target of reactive oxygen attack. Our data indicate that ROS perturbation of the mitochondria and dissipation of the electrochemical gradient is likely what causes the inhibition of StAR protein expression and, consequently, the inhibition of progesterone synthesis.
Our data indicate that StAR is posttranscriptionally inhibited by ROS. There also appears to be a constant level of the 37 kDa relative to the decreased 30- and 32-kDa forms (see especially Fig. 6, A and B). This finding suggests that processing and translocation of StAR at the mitochondria is disrupted by reactive oxygen treatment, which results in dissipation of m. How StAR facilitates cholesterol transfer across the mitochondrial intermembrane space is not completely understood. StAR is a nuclear-encoded, mitochondrial-targeted protein. Typical of most matrix-targeted proteins, StAR is translated as a larger molecular mass (37 kDa) precursor that contains mitochondrial targeting sequences in its amino terminus. Matrix targeting sequences are composed of a series of largely cationic amino acids that interact with the mitochondrial translocation complexes on the outer and inner mitochondrial membranes. The acidic nature of these sequences provides an ionic driving force that helps propel proteins bearing these sequences into the electronegative matrix. After StAR enters the matrix, it is proteolytically processed by matrix metaloproteases to the intermediate 32- and mature 30-kDa forms. Considerable evidence has been presented over the past several years in support of the hypothesis that the newly synthesized 37-kDa precursor form of StAR is the active form involved in cholesterol transfer (28, 44, 45, 46). The role of import and processing of StAR and its importance in cholesterol transfer remains controversial. However, it is generally accepted that the final intramitochondrial processing step rendering StAR as the 30-kDa mature form is the off step in the cholesterol transfer process. The cholesterol transfer activity of StAR has an absolute requirement for an intact m; indeed, the importance of m to StAR function and cholesterol transfer activity is unequivocal (44, 47, 48, 49, 50, 51, 52, 53). Our current study reports that oxidative stress causes the depolarization of the mitochondria and dissipation of m, resulting in concomitant inhibition of StAR protein expression and the inhibition of steroidogenesis, which confirms and extends these previous findings.
Disruption of the mitochondria and dissipation of the membrane potential often is associated with irreversible changes in mitochondria permeability that trigger a series of catabolic reactions resulting in apoptotic cell death (43). In this study, MA-10 cells exposed to concentrations of H2O2 as high as 250 µM, however, did not appear to undergo irreversible changes. There was no morphological evidence for apoptosis. Even though treatment with ROS resulted in dissipation of m, there was no appreciable loss of cell viability observed (Fig. 7). The trypan blue dye exclusion assay depends on intact cellular membranes as a measure of viability. These data indicate exposure to reactive oxygen treatments did not cause significant alterations in the plasma membrane. Lipid peroxidation is a well-established mechanism of nonspecific cellular injury leading to the production of lipid peroxides and their by-products such as malondialdehyde and 4-hydroxy-2(E)-nonenal. Measurement of malondialdehyde and 4-hydroxy-2(E)-nonenal provides a convenient index of lipid peroxidation. There was no apparent increase in the level of these lipid peroxidation products following exposure to ROS, as determined using the lipid peroxidation assay kit (Calbiochem, data not shown). Because there was no significant change in these lipid peroxidation products further indicates that overt damage to cellular membranes did not occur. Another widely used measure of cell viability is based on determination of cellular ATP levels (e.g. CellTiter-Glo viability assay, Promega Corp.; ApoSensor viability assay, BioVision, Mountain View, CA). As shown in Fig. 8, treatment with H2O2 did not affect cellular ATP levels, further supporting the conclusion that the effects of H2O2 were not due to cellular toxicity.
Removal of H2O2 and continued treatment with cAMP resulted in the partial restoration of StAR protein and progesterone production. Moreover, in cells exposed to prolonged treatment with H2O2 (for up to 6 h), we observed that steroidogenic function began to return to normal. These observations suggest that the effects of H2O2 are transient and the perturbation of the mitochondria resulted in a temporary loss of membrane potential. Considering that the effects of H2O2 were transient, it is even more striking how sensitive StAR protein is to loss of m that results from oxidative stress to the cells. Another consequence of long-term perturbation of m would be the inhibition of ATP production and decrease in cellular ATP levels.
In the present study, there was not a significant decrease in total cellular ATP observed as a result of H2O2 exposure (see Fig. 8). There is a significant decrease in ATP in cells treated with cAMP alone or cAMP plus xanthine/xanthine oxidase. These data contradict the study by Margolin et al. (23), who reported that treatment of rat granulosa cells with H2O2 resulted in a rapid and significant decrease in total cellular ATP levels. However, these investigators determined that inhibition of DNA repair activity during H2O2 exposure with 3-aminobenzamide prevented the H2O2-induced decrease in ATP levels. They concluded that changes in cellular ATP levels did not account for the inhibitory effects of H2O2 on granulosa cell FSH-stimulated progesterone production. Subsequently, they demonstrated that the effects of H2O2 were due to inhibition of the hormone-sensitive cholesterol transport into the mitochondria of rat luteal cells (22). The data we present here confirm these observations. First, because there is no significant decrease in total ATP levels, then depletion of total cellular ATP pools must not account for the inhibition of StAR. Second, our data demonstrate that the primary effect of H2O2 on the mitochondrial components of the steroidogenic machinery is on StAR protein because there is no change in P450scc protein. The earlier studies on the effects of oxidative stress on steroidogenesis from Behrman and Aten (22) and Stocco et al. (24), did not directly examine changes in StAR protein, and they did not assess changes in mitochondrial function.
The data we present in this study indicate that the dissipation of m that accompanies oxidative stress results in the inhibition of StAR protein expression and progesterone biosynthesis. Although total cellular ATP levels were not significantly altered during the time of ROS exposure in this study, it is likely that intramitochondrial levels of ATP were significantly diminished. To test this possibility, ATP levels in mitochondria isolated from oxidatively stressed MA-10 cells will need to be quantitated. Another possible consequence of dissipating m would be depletion of intramitochondrial Ca2+ levels. Mitochondrial [Ca2+] is regulated primarily by pump-leak mechanisms that depend on an intact electrochemical gradient for activity (54). A compelling body of work from Capponi and co-workers (55, 56, 57, 58, 59) has demonstrated a role for intramitochondrial Ca2+ in the regulation of StAR-mediated adrenal steroidogenesis. Investigations are currently underway to assess the relative contributions of intramitochondrial ATP and Ca2+ to the control of steroidogenesis in MA-10 cells.
Oxidative damage induced by ROS is implicated as an important contributing factor in the pathogenesis of more than 100 conditions (2). ROS-mediated perturbation of Leydig cell mitochondria resulting in inhibition of StAR protein expression and function may well be an important contributing factor to the decrease in testosterone associated with a host of pathological conditions, including inflammation, infection, ischemia-reperfusion injury, cryptorchidism, alcohol abuse, diabetes, and aging.
|
Acknowledgments |
|---|
The study has been previously presented in preliminary form at the 1st Congress of the European Academy of Andrology (EAA), March 2000, L’Aquila, Italy; the 95th Annual Meeting of the American Urological Association (AUA), May 2000, Atlanta, GA; and the 33rd Annual Meeting of the Society for the Study of Reproduction, July 2000, Madison, WI (60 ).
|
Footnotes |
|---|
Abbreviations: m, Mitochondrial membrane potential; 8-Br-cAMP, 8-bromo-cAMP; IOD, integrated OD; P450scc, P450 side-chain cleavage enzyme; ROS, reactive oxygen species; SFM, serum-free media; StAR, steroidogenic acute regulatory protein; TMRE, tetramethylrhodamine ethyl ester dye.
Received November 27, 2002.
Accepted for publication March 28, 2003.
|
References |
|---|
|
TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
|---|
in the regulation of mouse Leydig cell steroidogenesis. Endocrinology 132:2438–2444-hydroxylase/C17–20 lyase cytochrome P450 expression. Endocrinology 131:2165–2172-hydrosylase/C17–20 lyase in Leydig cells. Biol Reprod 42:399–404[Abstract]
-hydroxylase/C17–20 lyase in mouse Leydig cells: relation to steroid production. Mol Endocrinol 1:595–603This article has been cited by other articles:
 |
|
 |
|
  B. Piotrkowski, C. M Monzon, R. M Pagotto, C. G Reche, M. Besio, C. B Cymeryng, and O. P Pignataro Effects of heme oxygenase isozymes on Leydig cells steroidogenesis J. Endocrinol., October 1, 2009; 203(1): 155 - 165. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 C. Mondillo, R. M. Pagotto, B. Piotrkowski, C. G. Reche, Z. J. Patrignani, C. B. Cymeryng, and O. P. Pignataro Involvement of Nitric Oxide Synthase in the Mechanism of Histamine-Induced Inhibition of Leydig Cell Steroidogenesis via Histamine Receptor Subtypes in Sprague-Dawley Rats Biol Reprod, January 1, 2009; 80(1): 144 - 152. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 H. Chen, A. S. Pechenino, J. Liu, M. C. Beattie, T. R. Brown, and B. R. Zirkin Effect of Glutathione Depletion on Leydig Cell Steroidogenesis in Young and Old Brown Norway Rats Endocrinology, May 1, 2008; 149(5): 2612 - 2619. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 Z. Granot, O. Kobiler, N. Melamed-Book, S. Eimerl, A. Bahat, B. Lu, S. Braun, M. R. Maurizi, C. K. Suzuki, A. B. Oppenheim, et al. Turnover of Mitochondrial Steroidogenic Acute Regulatory (StAR) Protein by Lon Protease: The Unexpected Effect of Proteasome Inhibitors Mol. Endocrinol., September 1, 2007; 21(9): 2164 - 2177. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
D. C. Wathes, D. R. E. Abayasekara, and R. J. Aitken Polyunsaturated Fatty Acids in Male and Female Reproduction Biol Reprod, August 1, 2007; 77(2): 190 - 201. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
A. S. Midzak, J. Liu, B. R. Zirkin, and H. Chen Effect of Myxothiazol on Leydig Cell Steroidogenesis: Inhibition of Luteinizing Hormone-Mediated Testosterone Synthesis but Stimulation of Basal Steroidogenesis Endocrinology, June 1, 2007; 148(6): 2583 - 2590. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
P. Murugesan, M. Balaganesh, K. Balasubramanian, and J. Arunakaran Effects of polychlorinated biphenyl (Aroclor 1254) on steroidogenesis and antioxidant system in cultured adult rat Leydig cells J. Endocrinol., February 1, 2007; 192(2): 325 - 338. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
J. A. Allen, T. Shankara, P. Janus, S. Buck, T. Diemer, K. Held Hales, and D. B. Hales Energized, Polarized, and Actively Respiring Mitochondria Are Required for Acute Leydig Cell Steroidogenesis Endocrinology, August 1, 2006; 147(8): 3924 - 3935. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 A. Lacombe, V. Lelievre, C. E. Roselli, W. Salameh, Y.-h. Lue, G. Lawson, J.-M. Muller, J. A. Waschek, and E. Vilain Delayed testicular aging in pituitary adenylate cyclase-activating peptide (PACAP) null mice PNAS, March 7, 2006; 103(10): 3793 - 3798. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 L. Luo, H. Chen, M. A. Trush, M. D. Show, M. D. Anway, and B. R. Zirkin Aging and the Brown Norway Rat Leydig Cell Antioxidant Defense System J Androl, March 1, 2006; 27(2): 240 - 247. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 K. Shiraishi and K. Naito Increased expression of Leydig cell haem oxygenase-1 preserves spermatogenesis in varicocele Hum. Reprod., September 1, 2005; 20(9): 2608 - 2613. [Abstract] [Full Text] [PDF]
|
|
| |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
| Endocrinology | Endocrine Reviews | J. Clin. End. & Metab. |
| Molecular Endocrinology | Recent Prog. Horm. Res. | All Endocrine Journals |
