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Institute of Toxicology, Heinrich-Heine-Universität Düsseldorf, D-40225 Düsseldorf, Germany
2To whom correspondence should be addressed. E-mail: e.roehrdanz{at}bfarm.de.
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ABSTRACT |
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 TOP ABSTRACT INTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONLITERATURE CITED |
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KEY WORDS: • antioxidant enzymes • daidzein • expression • hepatoma cell • lipid peroxidation
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INTRODUCTION |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONLITERATURE CITED |
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–4
). Flavonoids in regularly consumed foods may also reduce the risk of death from coronary heart disease (5
,6
).
Several in vitro and animal studies were undertaken to clarify the biological and physiologic processes that account for the cancer chemoprotective effects of flavonoids. The estrogenic activities of the flavonoids may play an important role in their health-enhancing properties. Flavonoids have been reported to bind to estrogen receptors (ER)3
and prevent cell growth in hormone-dependent cancer cells (1
,7
,8
). Another proposed mechanism for cellular protection is the induction of phase II detoxification enzymes, leading to detoxification of proximate carcinogens generated by phase I metabolism. Indeed, some phytoestrogens were found to induce the phase II enzyme NADPH quinone reductase (9
). In addition to these different modes of action, the protective effects of flavonoids have been attributed mainly to their antioxidant properties. Flavonoids scavenge free radicals, chelate redox-active metal ions and increase metallothionein expression (10
–12
). Metallothionein can protect cells from heavy-metal toxicity, but also exerts antioxidant activity.
In the defense against oxidative stress, the antioxidant enzyme (AOE) system of cells plays an important role. The antioxidant enzymes include the superoxide dismutases (SOD), catalase and glutathione peroxidases (GPx) (13
–15
). Catalase and GPx convert H2O2 to H2O and the SOD catalyze the dismutation of the superoxide radical anion. There are three forms of SOD in mammals, i.e., MnSOD located in mitochondria, CuZnSOD found mainly in the cytosol and an extracellular SOD localized in the extracellular fluid.
The expression of AOE can be regulated by oxidative stress (16
–19
). Induction of catalase mRNA expression could be elicited by H2O2 or hyperoxia in different mammalian cells (16
–18
,20
). MnSOD expression was also found to be selectively induced by inflammatory mediators (21
,22
) as well as oxidative stress provoked either by H2O2 (17
,23
) or the redox-cycling compound paraquat (24
). However, little is known about the influence of flavonoids on the AOE system.
There are many reports relating to the reactivity of flavonoids with active oxygen species, thus emphasizing their antioxidant potential via a direct radical scavenging mechanism (10
,25
). On the other hand, flavonoids were found to induce the expression of enzymes such as metallothionein or NADPH quinone reductase, which may exert protective effects (9
,12
). We wanted to know whether flavonoids also can affect AOE expression, thus exerting indirect antioxidant activities. Therefore, we treated hepatoma cells with the flavonoid daidzein. We investigated the expression of different AOE and concurrently determined whether exposure of cells to daidzein protected against oxidative stress.
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MATERIALS AND METHODS |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONLITERATURE CITED |
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Rat hepatoma H4IIE cells were grown in Dulbecco’s modified Eagle’s medium (PAA Laboratories, Cölbe, Germany) and human hepatoma HepG2 cells in RPMI (PAA Laboratories) supplemented with 10% fetal calf serum, penicillin (1 x 105 U/L) and streptomycin (100 mg/L) in a humidified atmosphere of 5% CO2 in air at 37°C. Cells were seeded in 6-well plates. Unless stated otherwise, cells were treated for 24 h with different concentrations of daidzein, which was dissolved in dimethyl sulfoxide. The final concentration of the solvent never exceeded 0.7%. Control cells were treated with dimethyl sulfoxide. For the experiments involving H2O2 exposure, cells were pretreated for 24 h with daidzein in different concentrations. Then the medium was changed to one containing 2 mmol/L H2O2, and cells were incubated for another 6 h before malondialdehyde (MDA) measurement.
Viability assay.
To determine the viability of daidzein-treated cells, mitochondrial dehydrogenase activity was measured in the MTT-assay as described elsewhere (26
). Additionally, the Neutral Red assay was performed according to Borenfreund and Puerner (27
).
Lipid peroxidation.
Hepatoma H4IIE cells were pretreated with 200 or 300 µmol/L daidzein for 24 h followed by a 6-h treatment with 2 mmol/L H2O2. The respective controls received no treatment at all, were pretreated with medium and then with 2 mmol/L H2O2 or were given a daidzein pretreatment only. The amount of lipid peroxidation was determined by measuring the release of the breakdown product MDA into the medium. MDA was determined after reaction of cell culture supernatants with thiobarbituric acid and subsequent HPLC as previously described (24
). Measurements were compared with untreated control cells. In further experiments, H4IIE cells were exposed to different concentrations of daidzein only for 24 h and the amount of MDA released into the medium was determined
RNA isolation and RNA analysis.
Total RNA was isolated from cells using Trizol-Reagent (GIBCO BRL, Eggenstein, Germany). For Northern blot analysis, 5 µg of total RNA was resolved by electrophoresis in a 1% agarose, 2.25 mmol/L formaldehyde gel in a running buffer containing 20 mmol/L MOPS, pH 7, 0.5 mmol/L sodium acetate and 1 mmol/L EDTA. RNA was transferred to nylon membrane (Amersham, Arlington Height, IL) according to Maniatis et al. (28
) Purified cDNAs were labeled with [
32P] dCTP (111 TBq/mmol, Hartmann Analytic, Braunschweig, Germany) by random hexamer priming (Roche Diagnostics GmbH, Mannheim, Germany). Blots were prehybridized and hybridized with cDNAs for rat catalase, CuZnSOD and 18 S rRNA as described previously (24
). Autoradiographs were made by exposing blots to X-ray film (Kodak XAR) with an intensifying screen at -80°C. Blots were stripped and reprobed with the different cDNAs. Autoradiographs were analyzed by densitometric scanning using the Quantity One system from BIO RAD, Munich, Germany.
Polymerase chain reaction (PCR) after reverse transcription was performed for semiquantitative determination of MnSOD and glutathione peroxidase mRNA. Total RNA (1 µg) was transcribed into cDNA in a 25-µL final volume of reaction buffer (50 mmol/L Tris-HCL, 75 mmol/L KCL, 3 mmol/L MgCl2, 10 mmol/L dithiothreitol, 0.5 mmol/L of each dNTP) and 5 µmol/L oligo-d(T)16-primer, 1 U RNase inhibitor and 2.5 U MLV reverse transcriptase by incubation for 1 h at 42°C. The reaction was stopped by incubation at 99°C for 5 min. For rat MnSOD and GPx, PCR was performed with 100 ng of the synthesized cDNA as described elsewhere (29
,30
). GAPDH PCR was performed with 100 ng synthesized cDNA according to El-Bahay et al. (31
) The amplified PCR products were 394 bp for MnSOD mRNA, 602 bp for GPx mRNA and 450 bp for GAPDH mRNA. The conditions of PCR were set to be in the linear phase of amplification to allow for semiquantification of mRNA content. From each PCR reaction, 5 µL was electrophoresed in a 1% agarose gel in Tris-borate-EDTA buffer. The cDNA bands were visualized by UV illumination after the gels were stained with ethidium bromide. Gels were photographed and scanned densitometrically.
Transfection and reporter gene assays.
To evaluate the transcriptional control of the catalase gene, deletion plasmids were constructed from a plasmid containing 1.1 kb of the rat catalase upstream sequence (-1072 bp to +54 bp of transcription initiation site) in front of a luciferase expression vector (18
). The different promoter-reporter constructs of the catalase upstream region in front of the luciferase vector are shown in Figure 4
.
|
). Transfection cells were given fresh media 2–3 h before. Each well was cotransfected with 4 µg of a plasmid containing the luciferase reporter-construct and a plasmid containing the ß-galactosidase gene driven by the SV40 promoter (Promega, Mannheim, Germany). After 24 h, transfection cells were treated with 50 or 100 µmol/L daidzein for another 24 h. For harvesting, the cells were washed twice with 1 x PBS and then lysed in cell culture lysis buffer (Promega). Protein concentration of the cellular extract was determined according to Bradford (33
), using bovine serum albumin as standard. Cellular protein (10 µg) was used for luciferase assays. Luciferase activity was determined with a Multi-Biolumat LB 9505 C (Berthold, Bad Wildbad, Germany) using luciferase assay reagent according to the manufacturer’s protocol (Promega). With every transfection assay pGL3-basic and pGL3-control plasmid (Promega), containing SV 40 promoter and enhancer sequences, were transfected separately to additionally control for transfection efficiency. ß-Galactosidase activity was determined at 420 nm with o-nitrophenyl ß-D-galactopyranoside as substrate (28
). To minimize variability due to the difference in transfection efficiency among plates, the activity of luciferase and chloramphenicol acetyltransferase was corrected on the basis of the activity of ß-galactosidase. Statistical methods.
Results are expressed as means ± SEM. Significance was evaluated by ANOVA followed by Fisher’s Protected Least Significant Difference test. A probability of P < 0.05 was used as the criterion for significant difference.
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RESULTS |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONLITERATURE CITED |
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The cytotoxicity of daidzein was determined with two different assays (data not shown). In H4IIE cells, the MTT assay was more sensitive than the Neutral Red assay. According to the MTT test, cytotoxicity was apparent with 200 µmol/L daidzein. There was a significant reduction in viable cells of 
24%. This increased to 30% with 300 µmol/L daidzein and to 54% with 500 µmol/L daidzein. With the Neutral Red assay, cytotoxicity of daidzein became apparent (40% dead cells) and was significant when cells were exposed to 500 µmol/L daidzein.
Effect of daidzein on AOE expression in H4IIE cells.
H4IIE cells were grown to confluency and then treated with different concentrations of daidzein for 24 h. Figure 1A
shows the Northern blots for catalase and CuZnSOD mRNA expression and Figure 1
B the densitometric data relative to 18 S rRNA for catalase mRNA expression. In Figure 2A
, the PCR for detection of MnSOD and GPx is depicted and in Figure 2
B, the densitometric data relative to GAPDH mRNA expression. Daidzein treatment led to an increase of catalase mRNA expression (Fig. 1
B). With 300 µmol/L daidzein, a threefold increase in catalase mRNA levels was detected. With 300 µmol/L daidzein, we found a 100% increase in catalase activity (data not shown, mean of two experiments). On the basis of the Neutral Red assay, daidzein was not cytotoxic in this concentration range, whereas the MTT assay indicated minor cytotoxicity of daidzein with 24–30% dead cells. CuZnSOD mRNA expression was not affected by daidzein exposure; thus densitometric data are not shown. There was a slight, but significant 20% decrease in MnSOD mRNA expression after exposure of cells to 300 µmol/L daidzein (Fig. 2
B). An increase of 40% in Gpx mRNA expression generally occurred at all concentrations of daidzein tested except 200 µmol/L, and this difference was significant only at the highest concentration of daidzein, 300 µmol/L (Fig. 2
B).
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The promoter-reporter constructs for the catalase gene, as shown in Figure 3
, were transiently transfected into Hep G2 cells. Cells were then treated with different concentrations of daidzein for 24 h. In all of the experiments, the nontreated promoter-reporter constructs showed basal activity compared with the pGL3-basic plasmid. Figure 4
shows the luciferase activity of the transfected constructs after exposure to 50 or 100 µmol/L daidzein. In all promoter-reporter constructs tested, daidzein increased luciferase activity from one- to threefold. Interestingly, the promoter construct containing the whole 1.1-kb upstream region showed significantly lower inducible activity at a concentration of 50 µmol/L daidzein than the deletion constructs. The greatest increase in luciferase activity was observed for pLuc(-)2, which was about threefold after treatment of cells with 50 µmol/L daidzein.
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To determine whether the increase in catalase mRNA expression levels by daidzein exposure may exert antioxidant effects, H4IIE cells were pretreated with different concentrations of daidzein followed by a treatment with 2 mmol/L H2O2. The extent of lipid peroxidation was determined by measuring the release of the breakdown product MDA into the medium (Fig. 5A
). Treatment with 2 mmol/L H2O2 increased MDA levels only 3 times compared with controls. Daidzein pretreated cells were not protected from H2O2. On the contrary, MDA levels increased 4 times in these cells compared with controls and compared with the cells treated with H2O2 only. Treatment with 300 µmol/L daidzein alone increased MDA levels 50% compared with controls. Further experiments (Fig. 5
B) were performed to confirm this effect of daidzein on MDA levels. H4IIE cells were exposed to different concentrations of daidzein and the amount of MDA released into the medium was determined. An increase in MDA levels of 50% was detected in H4IIE cell supernatants treated with 200 or 500 µmol/L daidzein.
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DISCUSSION |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONLITERATURE CITED |
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); thus, they present a good model for these investigations.
The cytotoxicity of daidzein was measured with two different assays. The two highest concentrations of daidzein used for the evaluation of AOE expression levels were slightly cytotoxic in the MTT assay but nontoxic in the Neutral Red assay. The Neutral Red assay determines membrane uptake, whereas the MTT assay shows mitochondrial dehydrogenase activity (26
,27
). Obviously mitochondrial functions were first impaired by daidzein treatment, before a marked damage of cell membranes and thus the destruction of the whole cell became evident.
Daidzein treatment of hepatoma cells dramatically increased catalase mRNA expression. Kameoka et al. (12
) investigated catalase and CuZnSOD expression after daidzein treatment of CaCo2-cells and found no change in the expression pattern of either enzyme. This may have been due to the differences in cell lines because basal as well as inducible mRNA expression levels of AOE may differ depending on the cell type investigated (16
,22
,34
). To further elucidate the mechanisms underlying the increase in catalase mRNA by daidzein, we performed transfection experiments. Transfection of hepatoma cells with reporter genes containing different parts of the rat catalase upstream region and subsequent exposure to daidzein always resulted in an increase in reporter gene activity of treated compared with nontreated cells. These results clearly indicate that the increase of catalase mRNA after daidzein treatment is due to transcriptional activation of the rat catalase promoter. Little is known about transcriptional activation of the catalase gene. In general, post-transcriptional processes were found to be important for regulation of catalase gene expression. A redox-sensitive RNA binding protein was described for rat lung, which acts by increasing RNA stability (19
). In previous experiments, we found catalase gene induction to be regulated transcriptionally in hepatoma cells, whereas in hepatocytes, a translational mechanism was assumed (17
).
Isoflavonoids interact with ER. For daidzein, a stronger interaction with the ß- than the -subtype of the ER was shown (7
,35
). Similar in vitro interactions of phytoestrogens with human and rat ER and ERß have been reported, indicating that ER react similarly to phytoestrogens in the two species (7
,35
,36
). Azevedo et al. (37
) even found regulation of AOE to be dependent on sex steroids. Hepatoma cells such as those used for our experiments, however, are ER-negative, especially for later passages (38
). Thus, a transcriptional activation of the catalase promoter via ER interactions can be excluded.
To determine whether the increase in catalase expression protects the cells from oxidative damage, cells were pretreated with daidzein and then exposed to H2O2. Unexpectedly, in daidzein-pretreated cells, the oxidative damage, as measured via the lipid peroxidation product MDA, was more distinct than in cells treated with H2O2 only. Changes in the AOE mRNA expression pattern resulting from daidzein pretreatment may have led to an imbalance in the concerted action of the different AOE. This may have rendered the cells more sensitive toward the oxidative stress provoked by hydrogen peroxide treatment. Daidzein itself caused a mild oxidative stress. The antioxidant or prooxidant potential of flavonoids is a controversial topic in the literature (10
,39
). Increasing levels of daidzein were found to inhibit LDL oxidation in vitro (40
). Daidzein also protected against lecithin peroxidation induced by the superoxide anion generated through the xanthine-xanthine oxidase system (41
). On the other hand, in rat liver microsomes, daidzein was not able to inhibit enzymatically induced lipid peroxidation (42
). Hodgson et al. (43
) also found no in vivo antioxidant activity of daidzein. A number of flavonoids are able to produce reactive oxygen species by autoxidation and redox-cycling (44
). Similar mechanisms may be responsible for the oxidative stress we observed.
Oxidative stress was found to upregulate catalase mRNA expression in different cell lines as well as in neonatal rats under hyperoxic conditions (16
,19
). Different regulatory elements that play a role in the regulation of genes after oxidative stress have been identified (45
,46
). No consensus sequences of these well-described transcripton factors can be found in the catalase upstream region (see Fig. 4
). A putative AP2-sequence and a sequence resembling the binding site of the antioxidant responsive element are the only elements identified by sequence comparison so far. The truncated catalase-reporter-constructs showed a higher inducible reporter gene activity after exposure to 50 µmol/L daidzein than did the complete construct. Perhaps gene activity is suppressed by silencer elements present in the whole construct; such possible silencers were described by Takeuchi et al. (47
)
In addition to catalase, we also found an increase in GPx mRNA expression levels, which was not as distinct. In the 5'-flanking region of the human GPx gene, two cis-acting elements were characterized, which are of importance for gene regulation in an oxidative environment (48
). These elements were found to be active in human cardiomyocytes and HeLa cell cultures. The rat GPx gene likely is regulated similarly in H4IIE cells.
Surprisingly, there was a slight decrease in MnSOD mRNA expression after daidzein exposure. Induction of the MnSOD gene by tumor necrosis factor- and oxidative stress has been described in several studies (49
,50
). Daidzein is an efficient inhibitor of casein kinase II, which phosphorylates nuclear oncogene products and a number of proteins involved in gene expression (51
). It is possible that daidzein interferes with signal transduction pathways important for transcription of MnSOD.
In addition, CuZnSOD mRNA expression was not regulated coordinately with catalase and GPx expression. After daidzein exposure, no changes in CuZnSOD mRNA expression levels were detected. In previous studies, we (17
) and others (23
,52
) found that CuZnSOD often showed a stable expression pattern despite changes in the other AOE after exposure to different oxidants. This differential regulation of AOE expression is displayed after daidzein exposure as well.
In conclusion, our experiments showed that daidzein affected the AOE expression pattern. Interestingly, these changes did not add to the antioxidant, but rather to the oxidant properties of daidzein. The possible effect of phytoestrogens on human health may also be linked to the AOE system; as such, our in vitro studies suggest possible mechanisms of daidzein action. Further investigations will show whether daidzein has similar effects on the AOE system in vivo. Therefore, when evaluating the antioxidant capacity of flavonoids their ability to modulate AOE expression should also be considered.
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FOOTNOTES |
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3 Abbreviations used: AOE, antioxidant enzyme; CuZnSOD, copper zinc superoxide dismutase; ER, estrogen receptor; GPx, glutathione peroxidase; MDA, malondialdehyde; MnSOD, manganese superoxide dismutase; PCR, polymerase chain reaction; SOD, superoxide dismutase.
Manuscript received 30 August 2001. Initial review completed 3 October 2001. Revision accepted 14 December 2001.
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LITERATURE CITED |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONLITERATURE CITED |
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1. Adlercreutz, H., Mousavi, Y., Clark, J., Höckerstedt, K., Hämäläinen, E., Wählälä, K., Mäkela, T. & Hase, T. (1992) Dietary phytooestrogens and cancer: in vitro and in vivo studies. J. Steroid Biochem. Mol. Biol. 41:331-337.[Medline]
2. Lee, H. P., Gourley, L., Duffy, S. W., Esteve, J., Lee, J. & Day, N. E. (1991) Dietary effects on breast-cancer risk in Singapore. Lancet 337:1197-1200.[Medline]
3.
Severson, R. K., Nomura, A.M.Y., Grove, J. S. & Stemmermann, G. N. (1989) A prospective study of demographics, diet, and prostate cancer among men of Japanese ancestry in Hawaii. Cancer Res 49:1857-1860.
4.
Jenab, M. & Thompson, L. U. (1996) The influence of flaxseed and lignans on colon carcinogenesis and ß-glucuronidase activity. Carcinogenesis 17:1343-1348.
5.
Hertog, M.G.L., Kromhout, D., Aravanis, C., Blackburn, H., Buzina, R., Fidanza, F., Giampaoli, S., Jansen, A., Menotti, A., Nedeljikovic, S., Pekkarinen, M., Simic, B. S., Toshima, H., Feskens, E.J.M., Hollman, P.C.H. & Katan, M. B. (1995) Flavonoid intake and long-term risk of coronary heart disease and cancer in the seven countries study. Arch. Intern. Med. 155:381-386.
6.
Goodman-Gruen, D. & Kritz-Silverstein, D. (2001) Usual dietary isoflavone intake is associated with cardiovascular disease risk factors in postmenopausal women. J. Nutr. 131:1202-1206.
7.
Morito, K., Hirose, T., Kinjo, J., Hirakawa, T., Okawa, M., Nohara, T., Ogawa, S., Inoue, S., Muramatsu, M. & Masamune, Y. (2001) Interaction of phytoestrogens with estrogen receptors and ß. Biol. Pharm. Bull. 24:351-356.[Medline]
8. Dixon-Shanies, D. & Shaikh, N. (1999) Growth inhibition of human cancer cells by herbs and phytoestrogens. Oncol. Rep. 6:1383-1387.[Medline]
9. Wang, W., Liu, L. Q., Higuchi, C. M. & Chen, H. (1998) Induction of NADPH: quinone reductase by dietary phytoestrogens in colonic Colo205 cells. Biochem. Pharmacol. 56:189-195.[Medline]
10. Sichel, G., Corsaro, C., Scalia, M., Di Bilio, A. J. & Bonomo, R. P. (1991) In vitro scavenger activity of some flavonoids and melanins against O2-. Free Radic. Biol. Med. 11:1-8.[Medline]
11. Morel, I., Lescoat, G., Cogrel, P., Sergent, O., Pasdeloup, N., Brissot, P., Cillard, P. & Cillar, J. (1993) Antioxidant and iron-chelating activities of the flavonoids catechin, quercetin, and diosmetin on iron-loaded rat hepatocyte cultures. Biochem. Pharmacol. 45:13-19.[Medline]
12. Kameoka, S., Leavitt, P., Chang, C. & Kuo, S.-M. (1999) Expression of antioxidant proteins in human intestinal Caco-2 cells treated with dietary flavonoids. Cancer Lett 146:161-167.[Medline]
13. McCord, J. M. (1979) Superoxide, superoxide dismutase and oxygen toxicity. Hodgson, E. Bend, J. R. Philpot, R. M. eds. Reviews in Biochemical Toxicology 1979:109-124 Elsevier Amsterdam, The Netherlands. .
14. Aebi, H. (1984) Catalase in vitro. Methods Enzymol 105:121-126.[Medline]
15. Ursini, F., Maiorino, M., Brigelius-Flohé, R., Aumann, K. D., Roveri, A., Schomburg, D. & Flohé, L. (1995) Diversity of glutathione peroxidases. Methods Enzymol 252:38-114.[Medline]
16. Tate, D. J., Jr, Miceli, M. V. & Newsome, D. A. (1990) Phagocytosis and H2O2 induce catalase and metallothionein gene expression in human retinal pigment epithelial cells. Investig. Ophtalmol. Vis. Sci. 36:2856-2864.
17. Röhrdanz, E. & Kahl, R. (1998) Alterations of antioxidant enzyme expression in response to hydrogen peroxide. Free Radic. Biol. Med. 24:27-38.[Medline]
18. Röhrdanz, E., Schmuck, G., Ohler, S. & Kahl, R. (2001) The influence of oxidative stress on catalase and MnSOD gene transcription in astrocytes. Brain Res 900:128-136.[Medline]
19.
Clerch, L. B. & Massaro, D. (1992) Oxidation-reduction-sensitive binding of lung protein to rat catalase mRNA. J. Biol. Chem. 267:2853-2855.
20. Clerch, L. B. & Massaro, D. (1990) Perinatal rat lung catalase gene expression: influence of corticosteroid and hyperoxia. Am. J. Physiol. 260:L428-L433.
21.
Visner, G. A., Dougall, W. C., Wilson, J. M., Burr, I. A. & Nick, H. S. (1990) Regulation of manganese superoxide dismutase by lipopolysaccharide, interleukin-1, and tumor necrosis factor. J. Biol. Chem. 265:2856-2864.
22.
Wong, G.H.W. & Goeddel, D. V. (1988) Induction of manganous superoxide dismutase by tumor necrosis factor: possible protective mechanism. Science (Washington DC) 242:941-944.
23. Yoshioka, T., Homma, T., Meyrick, B., Takeda, M., Moore-Jarett, T., Kon, V. & Ichikawa, I. (1994) Oxidants induce transcriptional activation of manganese superoxide dismutase in glomerular cells. Kidney Int 46:405-413.[Medline]
24. Röhrdanz, E., Obertrifter, B., Ohler, S. & Kahl, R. (2000) Influence of adriamycin and paraquat on antioxidant enzyme expression in primary rat hepatocytes. Arch. Toxicol. 74:231-237.[Medline]
25. Hanashi, Y., Ogawa, S. & Fukui, S. (1994) The correlation between active oxygen scavenging and antioxidative effects of flavonoids. Free Radic. Biol. Med. 16:845-850.[Medline]
26. Mosmann, T. (1983) Rapid colorimetric assay for cellular growth and survival: application to proliferation and cytotoxicity assays. J. Immunol. Methods 65:55-63.[Medline]
27. Borenfreund, E. & Puerner, J. A. (1985) Toxicity determined in vitro by morphological alterations and neutral red absorption. Toxicol. Lett. 24:119-124.[Medline]
28. Maniatis, T., Fritsch, E. F. & Sambrook, J. (1982) Molecular Cloning: A Laboratory Manual 1982 Cold Spring Harbor Laboratory New York, NY. .
29. Röhrdanz, E., Schmuck, G., Ohler, S., Tran-Thi, Q.-H. & Kahl, R. (2001) Changes in antioxidant enzyme expression in response to hydrogen peroxide in rat astroglial cells. Arch. Toxicol. 75:150-158.[Medline]
30. Springer, L. N., Tilly, J. L., Sipes, I. G. & Hoyer, P. B. (1996) Enhanced expression of bax in small preantral follicles during 4-vinylcyclohexene diepoxide-induced ovotoxicity in the rat. Toxicol. Appl. Pharmacol. 139:402-410.[Medline]
31.
El-Bahay, C., Gerber, E., Horbach, M., Tran-Thi, Q.-H. & Röhrdanz, E. (1999) Influence of tumor necrosis factor- and silibin on the cytotoxic action of -amanitin in rat hepatocyte culture. Toxicol. Appl. Pharmacol. 158:253-260.[Medline]
32.
Gorman, C. M., Moffat, L. F. & Howard, B. H. (1982) Recombinant genomes which express chloramphenicol acetyltransferase in mammalian cells. Mol. Cell. Biol. 2:1044-1051.
33. Bradford, M. M. (1976) A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal. Biochem. 72:248-254.[Medline]
34. Yoo, J.-H., Erzurum, S. C., Hay, J. G., Lemarchand, P. & Crystal, R. G. (1994) Vulnerability of the human airway epithelium to hyperoxia. J. Clin. Investig. 93:297-302.
35.
Casanova, M., You, L., Gaido, K. W., Archibeque-Engle, S., Janszen, D. B. & Heck, d’A. H. (1999) Developmental effects of dietary phytoestrogens in Sprague-Dawley rats and interactions of genistein and daidzein with rat estrogen receptors and ß in vitro. Toxicol. Sci. 51:236-244.
36. Nikov, G. N., Hopkins, N. E., Boue, S. & Alworth, W. L. (2000) Interactions of dietary estrogens with human estrogen receptors and the effect on estrogen receptor-estrogen response element complex formation. Environ. Health Perspect. 108:867-872.[Medline]
37. Azevedo, R. B., Lacava, Z.G.M., Miyasaka, C. K., Chaves, S. B. & Curi, R. (2001) Braz. J. Med. Biol. Res. 34:683-687.
38.
Archer, T. K., Tam, S. P., Deugau, K. V. & Deeley, R. G. (1985) J. Biol. Chem. 260:1676-1681.
39. Van Acker, S.A.B.E., de Groot, M. J., van den Berg, D.-J., Tromp, M.N.J.L., Donné-Op den Kelder, G., van der Vijgh, W.J.F. & Bast, A. (1996) A quantum chemical explanation of the antioxidant activity of flavonoids. Chem. Res. Toxicol. 9:1305-1312.[Medline]
40. Hwang, J., Sevanian, A., Hodis, H. N. & Ursini, F. (2000) Synergistic inhibition of LDL oxidation by phytoestrogens and ascorbic acid. Free Radic. Biol. Med. 29:79-89.[Medline]
41. Toda, S. & Shirataki, Y. (1999) Inhibitory effects of isoflavones on lipid peroxidation by reactive oxygen species. Phytother. Res. 13:163-165.[Medline]
42. Sato, T., Kawamoto, A., Tamura, A., Tatsumi, Y. & Fujii, T. (1992) Mechanism of antioxidant action of pueraria glycoside (PG)-1 (an isoflavonoid) and magniferin (a xanthonoid). Chem. Pharm. Bull. 40:721-724.
43. Hodgson, J. M., Puddey, I. B., Croft, K. D., Mori, T. A., Rivera, J. & Beilin, L. J. (1999) Isoflavonoids do not inhibit in vivo lipid peroxidation in subjects with high-normal blood pressure. Atherosclerosis 145:167-172.[Medline]
44. Canada, A. T., Giannella, E., Nguyen, T. D. & Mason, R. P. (1990) The production of reactive oxygen species by dietary flavonols. Free Radic. Biol. Med. 9:441-449.[Medline]
45.
Baeuerle, P. A. (1991) The inducible transcription activator NF-
B: regulation by distinct protein subunits. Biochim. Biophys. Acta 1072:63-80.[Medline]
46.
Rushmore, T. H., Morton, M. R. & Pickett, C. B. (1991) The antioxidant responsive element. Activation by oxidative stress and identification of the DNA consensus sequence required for functional activity. J. Biol. Chem. 266:11632-11639.
47.
Takeuchi, T., Nakamura, S., Kayasuga, A., Isa, S. & Sato, K. (2000) Multiple elements for negative regulation of the rat catalase gene expression in dedifferentiated hepatoma cells. J. Biochem. 128:1025-1031.
48.
Cowan, D. B., Weisel, R. D., Williams, W. G. & Mickle, D.A.G. (1993) Identification of oxygen responsive elements in the 5'-flanking region of the human glutathione peroxidase gene. J. Biol. Chem. 268:26904-26910.
49.
Kuo, S., Cheswron, S. E., Mellott, J. K., Rogers, R. J., Hsu, J.-L. & Nick, H. S. (1999) In vivo architecture of the manganese superoxide dismutase promoter. J. Biol. Chem. 274:3345-3354.
50.
Xu, Y., Kiningham, K. K., Devalaraja, M. N., Yeh, C.-C., Majima, H., Kasarskis, E. J. & St Clair, D. K. (1999) An intronic NF-B element is essential for induction of the human manganese superoxide dismutase gene by tumor necrosis factor- and interleukin-1ß. DNA Cell Biol 18:709-722.[Medline]
51.
Allende, J. E. & Allende, C. C. (1995) Protein kinases. 4. Protein kinase CH2: an enzyme with multiple substrates and a puzzling regulation. FASEB J. 9:313-323.
52.
Dougall, W. C. & Nick, H. S. (1991) Manganese superoxide dismutase: a hepatic acute phase protein regulated by interleukin-6 and glucocorticoids. Endocrinology 129:2376-2384.
53.
Toda, S., Takeuchi, T., Hori, N. & Sato, K. (1997) Inverted repeats in the TATA-less promoter of the rat catalase gene. J. Biochem. 121:1035-1040.
54. Van Remmen, H., Williams, M. D., Yang, H., Walter, C. A. & Richardson, A. (1998) Analysis of the transcriptional activity of the 5'-flanking region of the rat catalase gene in transiently transfected cells and transgenic mice. J. Cell. Physiol. 174:18-26.[Medline]
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P < 0.05 vs. pLuc1 treated with 50 µmol/L daidzein.
