Abstract
Reactive oxygen species (ROS) play a pivotal role in UVA-induced cell damage. As expression of the inducible nitric oxide synthase (iNOS) is a normal response of human skin to UV radiation we examined the role of nitric oxide (NO) as a protective agent during or even after UVA1- or ROS-exposure against apoptosis or necrosis of rat endothelial cells. When added during or up to 2 h subsequent to UVA1 or ROS exposure the NO-donor S-nitroso-cysteine (SNOC) at concentrations from 100–1000 μM significantly protects from both apoptosis as well as necrosis. The NO-mediated protection strongly correlates with complete inhibition of lipid peroxidation (sixfold increase of malonedialdehyde formation in untreated versus 1.2-fold with 1 mM SNOC). NO-mediated protection of membrane function was also shown by the inhibition of cytochrome c leakage in UVA1 treated cells, a process not accompanied by alterations in Bax and Bcl-2 protein levels. Thus, the experiments presented demonstrate that NO exposure during or even after a ROS-mediated toxic insult fully protects from apoptosis or necrosis by maintaining membrane integrity and function.
Similar content being viewed by others
Introduction
Ultraviolet radiation is divided into three regions: UVC (190–290 nm), UVB (290–320 nm) and UVA (320–400 nm). Effects on cells by UV radiation of shorter wavelengths, UVB and UVC, have been extensively investigated in terms of direct effects on DNA.1 UVA was initially perceived as innocuous to skin however, numerous reports recently have demonstrated cytotoxic effects after exposure of eukaryotic cells to UVA radiation as a consequence of oxidative stress. UVA-induced oxidative damage has been reported for several target molecules as well as organelles.2,3
A plethora of anti-oxidant and anti-apoptotic defense mechanisms exists in mammalian cells, such as enzymes or compounds which quench or remove reactive oxygen species (ROS), proteins with chaperone activity such as heat shock proteins4 or proteins of the bcl-2 family which have been shown to serve as potent anti-apoptotic factors.5 Recent evidence suggests that the signal molecule nitric oxide (NO) can also act as an antiapoptotic agent.6 NO and equivalent amounts of citrulline are synthesized from the guanidino nitrogen of L-arginine by NO synthases (NOS) found in endothelial cells, neurons and upon activation by proinflammatory stimuli in most cell types. The NOS enzyme family consists of three isoenzymes: constitutively expressed and calcium/calmodulin-regulated are the endothelial (ecNOS) and the neuronal (ncNOS) isoenzymes which produce regulated low amounts of NO for short periods of time, whereas the cytokine-inducible and calcium-independent isoenzyme (iNOS) synthesizes NO for extended periods of time.7,8
Cytokines are known modulators of endothelial cell functions during inflammatory processes. One prominent effect that cytokines can exert in endothelial cells is the induction of iNOS and thus high-output NO synthesis.9 Recently, we have shown that exposure well before UVA1-irradiation of endothelial cells to NO either endogenously synthesized by iNOS after challenge by proinflammatory cytokines or applied exogenously in the form of a NO-donor fully protects cells from UVA1-induced cell damage. The protective effect strongly correlated with a NO-induced increase in Bcl-2 protein expression.10 As in the vivo situation NO-generation by iNOS will start after skin exposure to sunlight, we now tested whether and by which mechanisms a protection after UV-irradiation is exerted. We show a strong protective effect of NO even when added during or up to 2 h after the toxic insult. This timing does not allow for increased Bcl-2 expression and we here demonstrate that nitric oxide acts as a powerful inhibitor of ROS-mediated lipid peroxidation with a concomitant arrest of Bax and Bcl-2 independent mitochondrial cytochrome c release. Thus data provide further evidence for the protective role of NO synthesis in skin helping to prevent cellular damage after UV-exposure.
Results
Characterization of endothelial cell death pathways
Irradiation of EC with UVA1 leading to endothelial apoptotic cell death in a dose-dependent manner has been described previously.10 Using irradiation with a dose of 10 J/cm2 UVA, the appearance of apoptotic markers becomes significant after a delay of 4–8 h (Figure 1A) as quantified by Hoechst staining and in situ nick translation. In addition, UVA1-induced cell death is completely inhibited by incubation with the caspase inhibitor Z-VAD (Figure 1B) as additional prove for apoptosis.
We also treated cells with singlet oxygen, generated by photoexcitation after pre-loading with Rose Bengal (RB/hν). Dependent on the concentration of Rose Bengal cell death was maximal at 1.8 μM RB/hν, with half maximal induction of cell death at 0.9 μM RB/hν (Figure 2A). Interestingly, the mode of cell death was necrosis exclusively as evidenced by the rapid onset of cell death which was nearly complete after 2–4 h (Figure 2B) but also by the complete lack of apoptotic nuclear morphology as well as failure of protection by the caspase inhibitor Z-VAD (Figure 2C). Because of its lipophilic character, incubation of endothelial cells with Rose Bengal led to its enrichment into intracellular membranes predominantly11 (Figure 2D).
Protection by antioxidative agents
Adding various antioxidants we elucidated the role of ROS during UVA1-irradiation or Rose Bengal treatment. Agents were added to cell cultures during UVA1-irradiation or RB/hν treatment and the numbers of viable cells were determined after 24 h of culture. Deuterium oxide (D2O) prolonging the lifetime of 1O2 significantly enhanced EC death after UVA1-irradiation or RB/hν-challenge. Conversely, compounds quenching singlet oxygen, i.e. NaN3 (20 mM), histidine (40 mM), and imidazole (40 mM) exerted a significant protection (Figure 3A) suggesting the involvement of singlet oxygen generation early in UVA1-induced cell death, as has been reported previously.3,12,13 All four compounds gave the same exacerbation or augmentation also in RB/hν-induced toxicity. Next the involvement of superoxide anion generation was screened by adding the O2.−-quencher MnTBAP (80 μM) or DETC (1 mM), an inhibitor of the intracellular SOD. Both, O2.−-depletion by MnTBAP or inhibition of its conversion by SOD to H2O2 fully protected cells from induced apoptosis or necrosis (Figure 3B). In contrast, addition of SOD (1000 U/ml) significantly enhanced cell death, while heat-inactivated SOD was without effect (Figure 3B) indicating that H2O2 more than O2.− may represent the toxic agent during UVA-irradiation or RB/hν-treatment. This is supported by our findings that addition of catalase (2000 U/ml) during the toxic inputs was fully protective, whereas the catalase inhibitor 3-amino-1,2,4-triazole (500 μM) enhanced cytotoxicity (Figure 3C). The antioxidant BHT (10 μM), an strong inhibitor of lipid peroxidation, fully protects (Figure 3D) whereas neither DMSO (100 mM) nor mannitol (100 mM) both scavenging of OH. influenced cell death rates indicating that OH. appears not to contribute to UVA1-or RB/hν-induced cell death (data not shown).
Exogenous NO present during the experimental procedure fully protects from both apoptosis caused by UVA1 and necrosis caused by singlet oxygen
We had shown previously that the presence of NO for 24 h prior to UVA fully protected cells from apoptosis.10 We now investigated whether NO could also protect when present during treatment and whether it would exacerbate or augment RB/hν-induced necrosis. During UVA treatment cells were incubated with the NO donors SNOC or DETA/NO or with the respective controls cysteine or DETA. SNOC, in a concentration-dependent manner, lowered or completely inhibited UVA1-induced apoptosis as well as RB/hν-induced necrosis of EC. Concentrations of SNOC ⩾100 μM exerted substantial protection (Figure 4A,B), with best results found with 1 mM SNOC, whereas the control compound cysteine was without effect (Figure 4A,B). Experiments using the NO donor DETA/NO gave similar results (Figure 4C,D).
Time window for protection by nitric oxide or antioxidants added after the insults
To examine whether the various agents tested will also protect when added after UVA1-irradiation or singlet oxygen treatment, antioxidants or nitric oxide were added to EC cultures at different time points after the treatments.
After UVA1-irradiation (Figure 5A) or Rose Bengal-challenge (Figure 5B), NaN3 (20 mM) ceased to protect when added as early as 5 min after UVA1. MnTBAP (80 μM) showed a significant protection when added up to 15 min after the toxic stimuli. In contrast, catalase (2000 U/ml) or BHT (10 μM) show comparable time-courses of protection which is significant when added to cell cultures as late as 2 h after UVA1-challenge or 1 h after RB/hν-treatment. Examining the protective time window for NO by addition of the NO-donor SNOC (1 mM) at different time intervals after UVA1-irradiation (Figure 5A) or RB/hν treatment (Figure 5B) we find a similar time window for protection against UVA1-induced apoptosis or 1O2-induced necrosis, which parallels the protection seen after incubation with catalase or BHT.
Protection by NO is not due to reaction with or quenching of ROS
Using dihydrorhodamine 123 (10 μM) a fluorescent dye for H2O2 detection we examined the input of NO as potential quencher or reaction partner of the ROS formed after UVA1-irradiation (8 J/cm2) or 1O2 generation (1.5 μM RB/hν). UVA1-exposure of otherwise untreated EC (Figure 6A) led to an increase in intracellular fluorescence (Figure 6B). In contrast, presence of 1O2 quenchers (Figure 6C, histidine, 40 mM), inhibition of endogenous SOD with 1 mM diethyldithiocarbamate (Figure 6D), O2.− depletion by 80 μM MnTBAP (Figure 6F) or H2O2 depletion by 2000 U/ml catalase (Figure 6G) fully inhibited rhodamine 123 formation, whereas heat-inactivated catalase had no inhibitory effect (Figure 6H). In contrast, neither the presence of 10 μM BHT (Figure 6I) nor of 1 mM SNOC (Figure 6J) inhibited the UVA1-or the RB/hν-induced fluorescence, suggesting that neither BHT nor NO will react directly with the ROS species involved. Control incubations of irradiated cells with SNOC or any of the other substances used (data not shown) did not result in increased cellular fluorescence, while incubation of cells with H2O2 (0.3 mM for 15 min) resulted in a pronounced fluorescence signal (Figure 6L). Besides reacting with H2O2, dihydrorhodamine 123 may also react with peroxynitrite a reaction product of NO and O2−..14 To validate this possibility we incubated UVA or Rose Bengal treated cells with a SOD inhibitor exactly as already shown in Figure 6D but in the presence of the NO-donor SNOC (1 mM). As shown in Figure 6K, no apparent increase in mitochondrial fluorescence could be observed further corroborating the notion that under the conditions used peroxynitrite will not be produced. Results obtained with the RB/hν-system were similar (data not shown).
Nitric oxide fully protects from hydrogen peroxide induced toxicity
Data presented above indicate that H2O2 formed enzymatically or non-enzymatically from 1O2 or O2.− may represent a late ROS product involved in cell death mediated by UVA1-irradiation or 1O2-challenge. Thus, we examined the effects of exogenously applied nitric oxide (1 mM DETA/NO) or catalase (4000 U/ml) on H2O2-induced endothelial cell death, respectively. Incubation of endothelial cells with H2O2 for 24 h (Figure 7A) led to concentration-dependent cell death. Maximal toxicity was detected after incubation with 0.9 mM, half-maximal with 0.7 mM H2O2. Hydrogen peroxide-induced cell death was strongly reduced in the presence of catalase as well as in the presence of DETA/NO, whereas the controls DETA alone or heat-inactivated catalase had no effects.
Furthermore, with the half-maximal toxic dose of 0.7 mM H2O2 DETA/NO was protective even when added 90 min after the toxic stimulus, whereas with the maximal dose of 0.9 mM H2O2 DETA/NO at a concentration of 1 mM was not efficient enough to protect from cell death (Figure 7B).
NO inhibits lipid peroxidation
The results presented so far suggest lipid peroxidation as a crucial step in cell destruction. Therefore, endothelial cells were treated in the absence or presence of the various additives and lipid peroxidation was analyzed by determining the amount of malonedialdehyde formed. Results show a close correlation between UVA1- or H2O2-induced apoptosis or RB/hν-induced necrosis and lipid peroxidation: As demonstrated in Figure 8A, UVA1-irradiation as well as 1O2 generation from RB/hν led to a highly significant increase in endothelial lipid peroxidation as evidenced by the amount of MDA formation. All substances which were shown to protect from apoptosis or necrosis (1 mM SNOC, 20 mM NaN3, 10 μM BHT, 2000 U/ml catalase, 1 mM DETC, 80 μM MnTBAP) fully protected from lipid peroxidation. In addition, promoting induced cell death by addition of SOD or D2O further enhanced lipid peroxidation, whereas the control compounds did not affect the levels of lipid peroxidation. Furthermore, incubation of endothelial cells with H2O2 (0.9 mM) led to an approximately eightfold increase in lipid peroxidation, whereas incubation with hydrogen peroxide in the presence of 1 mM DETA/NO, 10 μM BHT or 2000 U/ml catalase significantly reduced formation of lipid peroxides to control values, respectively (Figure 8B).
We also examined the role of NO as an inhibitor of lipid peroxidation in a cell-free model using liposomes and the 1O2 releasing endoperoxide NDPO2 (20 mM) as an inducer of lipid peroxidation. As exogenous NO source we used the NO donor MAHMA/NO (5 mM). Thermal decomposition of NDPO2 at 37°C led to a significant 6–11-fold increase in lipid peroxidation which was completely inhibited by the NO-donor MAHMA/NO, while MAHMA had no effect (Figure 8C).
Inhibition of lipid peroxidation by NO also protects from UVA1-induced mitochondrial cytochrome c release
For further elucidation of the molecular mechanism responsible for the antiapoptotic effects of NO present during UVA1-exposure (8 J/cm2), we examined events upstream of the caspase cascade. Using the Western blot technique we investigated the expression of the apoptosis relevant proteins Bcl-2 and Bax as well as the release of holocytochrome c from mitochondria into the cytoplasm as an early and pivotal signal in initiation of the apoptosis program. As shown in Figure 9A, UVA1-irradiation does not influence the amount of Bax protein. More importantly, during the time interval examined we find no increases of Bcl-2 protein expression and a caspase-mediated cleavage of the antiapoptotic Bcl-2 could not be demonstrated within the first 4 h after UVA1-irradiation (Figure 9B). In contrast, 2 h after UVA1-irradiation we found holocytochrome c appearing in the cytoplasmic compartment and this remained for up to 4 h after UVA1-challenge (Figure 10A). Importantly, as shown in Figure 10B, this holocytochrome c release was completely blocked when UVA1-irradiation of endothelial cells was performed in the presence of SNOC or any of the antioxidants, shown to inhibit lipid peroxidation (1 mM SNOC, 40 mM histidine, 80 μM MnTBAP, 2000 U/ml catalase), whereas the control compounds did not block the increases in holocytochrome c release.
Discussion
The cytotoxic action of UVA1-radiation on mammalian cells is known to depend on the presence of oxygen. Multiple evidence exist that reactive oxygen species are involved.15 Studies with chemical probes have implicated the involvement of H2O2,16 O2−.,17 OH.,18 and an important role for 1O213 in UVA1-mediated cytotoxicity. In biological environments singlet oxygen is highly reactive with a sufficiently long half-life to reach specific compartments.19 All ROS are potentially harmful to cells as they interact with and modify a broad spectrum of biomolecules.20 Thus, exposure of cells to ROS results in progressive cell damage by oxidative modification of various bio-molecules.21
Free-radical-induced damage of membranes results in loss of membrane function caused by UVA1-radiation as well as radical-induced membrane damage using insults other than UVA1 radiation22,23 correlates with cell death via apoptosis or necrosis. We recently observed that UV-challenge of normal human skin leads to the induction of iNOS expression in keratinocytes and capillary endothelial cells.24 High amounts of NO as produced by iNOS are known inducers of cell death via apoptosis or necrosis determined by the energy status of the respective cell.25,26 Thus, it was tempting to speculate that iNOS expression after UV challenge may contribute to cellular skin damage.
However, NO may also exert antiapoptotic activity and indeed we have shown recently, that the presence of endogenously or exogenously formed NO prior to UVA1-irradiation results in a strong increase of Bcl-2 protein expression correlating with full protection from UVA1-induced apoptosis.10 We now provide evidence for protection even when NO is added up to 2 h after irradiation and also present data showing that here a different mechanism upstream of the apoptotic machinery is at work.
The time-course experiments using various antioxidants implicate a ROS cascade starting with UVA1-or Rose Bengal-induced 1O2 formation, followed by generation of O2−., then H2O2 accumulation, and the latest step found to occur in our experiments was lipid peroxidation. Interestingly, and despite the close similarity of the chain of ROS formation both ultimately resulting in lipid peroxidation, the mode of cell death differs for the two types of treatment. This may be due to the lipophilic character of Rose Bengal which readily incorporates into cellular membranes. Thus, 1O2 formation and subsequent reactions will occur within bio-membranes and may thus lead to rapid and irreversible destruction of membrane integrity, which is regarded as the hallmark event of necrosis. In contrast, UVA1 irradiation will lead to 1O2 formation in many compartments of the cell mostly dependent on the presence of intracellular chromophores responsible for 1O2 release.27,28 As long as energy equivalents are not leaking from the cytoplasm as is the case with necrosis, cells can undergo apoptosis as has been reported.25 It thus appears that here the decision for death by necrosis or apoptosis is not dominated by the type of molecular insult, but rather by the site of the damaging event.
Lipid peroxidation, found to represent a late step in the cascade, was decreased by the various antioxidants used as well as by exogenously applied NO donors, all of which inhibit the onset of necrosis or apoptosis. Examining events downstream of lipid peroxidation demonstrated a close positive correlation between the peroxidation of lipids and mitochondrial cytochrome c leakage. Within the time frame given, UVA1-irradiation in the presence or absence of NO does neither decrease nor increase Bcl-2 protein expression or caspase mediated Bcl-2 cleavage, nor does the late addition of NO allow for gene up-regulation. Thus, in this experimental setup protection from cytochrome c release by acute NO treatment strongly correlates with, and thus appears to be dominantly mediated by inhibition of lipid peroxidation.
Lipid peroxidation results from the net abstraction of an allylic hydrogen atom of an unsaturated fatty acid by an initiating radical species to generating a lipid radical. The lipid radical then reacts with O2 to generate an alkylperoxy radical (LOO.) which can further react with another lipid to form another lipid radical that can also react with O2 and so on.29 Thus, a single initiating event can lead to the destruction/modification of numerous lipid molecules resulting in loss of membrane integrity. As shown, lipid peroxidation can be avoided or limited by inhibiting the generation of or quenching the initiating radical species by antioxidants, however, data presented do not corroborate such a role for NO but rather suggest a radical-chain terminating activity. The NO-radical (.NO) reacts rapidly via simple radical-radical combination reactions with species possessing unpaired electrons as .O2, O2 and O2.−. The ability of NO to quench other radical species also allows it to terminate radical chain reactions.30 The reaction of .NO with LOO. species readily predominates over the much slower initiation of secondary peroxidation propagation reactions by LOO. with vicinal unsaturated lipids, and when inhibiting lipid peroxidation propagation reactions, NO undergoes an initial termination reaction with organic peroxyl radicals to form organic peroxynitrates (LOONO).31
In summary, we present evidence that NO can prevent cell death as a consequence of UVA-induced onset of lipid peroxidation and ROS-formation. This finding bears significance in understanding protective responses in human skin exposed to excessive doses of sunlight. As during the first exposure to UV skin cells are usually not expressing iNOS, it is important to understand the protective mechanisms exerted by subsequent NO synthesis in the skin, a process which will help to minimize skin cell destruction.
Materials and Methods
Reagents
Endothelial cell growth supplement (ECGS), Neutral Red, deuterium oxide (98%), rabbit anti-human von Willebrand Factor (vWF) antiserum, monoclonal mouse anti-α-tubulin antibody, Rose Bengal, histidine, mannitol, imidazole, dimethyl sulfoxide (DMSO), sodium azide, catalase, diethyldithiocarbamate (DETC), 3-amino-1,2,4-triazole (ATA), H2O2, and Hoechst dye H33342 were purchased from Sigma (Deisenhofen, Germany), rabbit anti-rat Bcl-2 antibody or rabbit anti-rat Bax antiserum from Pharmingen (San Diego, CA, USA), peroxidase-conjugated porcine anti-rabbit IgG from DAKO (Hamburg, Germany), and peroxidase-conjugated goat anti-mouse IgG from Zymed Laboratories (San Francisco, CA, USA), manganese (III) tetrakis(4-benzoic acid)porphyrin (MnTBAP), and manganese (III) tetrakis(1-methyl-4-pyridyl)porphyrin (MnTMPyP) from Alexis (Läufelfingen, Switzerland), diethylenetriamine and 2,[6]-di-tert-butyl-p-cresol (butylated hydroxytoluene, BHT) from Aldrich (Steinheim, Germany), dihydrorhodamine 123 (DHR) from Molecular Probes (Eugene, OR, USA), the monoclonal antibody O×43 from Serotec (Camon, Wiesbaden, Germany), and the monoclonal mouse anti-holocytochrome c antibody from R&D Systems (Heidelberg, Germany), protease inhibitor mix, trypsin, EDTA, fetal calf serum (FCS, endotoxin free), RPMI-1640 (endotoxin free), NADP, glucose-6-phosphate, glucose-6-phosphate dehydrogenase from Boehringer Mannheim (Mannheim, Germany) or Gibco Laboratories (Eggenstein, Germany), and the ICE-inhibitor Z-VAD from Enzyme Systems (Livermore, CA, USA). The endoperoxide 3,3′-(1,4-naphthylidene)dipropionate (NDPO2) was synthesized as described by Di Mascio and Sies.32 The NO donors (Z)-1-[N-(2-aminoethyl)-N-(2-ammonioethyl)amino]diazen-1-ium-1,2-diolate (DETA/NO), (Z)-1-{N-methyl-N-[6-(N-methylammoniohexyl)amino]}diazen-1-ium-1,2-diolate (MAHMA/NO), and S-nitrosocysteine (SNOC) were synthesized as described previously.33,34 The iNOS inhibitor L-N5-(1-iminoethyl)-ornithin (NIO) was a kind gift from Boehringer Mannheim. As UVA1-source we used a Sellas-2,000 or Sellas-4000 lamp (Sellas Medizinische Geräte, Gevelsberg, Germany) emitting the UVA1-spectrum (340–390 nm).
Endothelial cells
Endothelial cells (EC) were isolated by outgrowth from male Wistar rat aortic rings as described previously.9 Briefly, aortic segments were placed on top of a collagen gel (1.8 mg collagen/ml) in 24-well tissue culture plates and incubated in RPMI 1640/ 20% FCS supplemented with 100 μg ECGS/ml for 5 days. Aortic explants were then removed, cells detached with 0.25% collagenase in HBSS and replated onto plastic culture dishes in RPMI 1640/ 20% FCS. Cells were subcultured for up to eight passages, and removal from culture dishes for each passage was performed by treatment with trypsin/EDTA. Cellular characterization of cultured endothelial cells was performed by determination of the endothelium characteristic antigenic phenotype using the anti-vWF antiserum, the endothelium-specific monoclonal antibody O×43, and the respective peroxidase-conjugated secondary antibodies as described previously.35
Singlet oxygen production
Intracellular release of singlet oxygen was achieved by photoexcitation of solutions containing endothelial cells and varying concentrations of Rose Bengal (RB/hν) with a commercially available white lamp from a fixed distance.36 Briefly, endothelial cells were incubated for 15 min with Rose-Bengal in the dark at 37°C in RPMI 1640 without FCS and phenol red. Cells were then irradiated for 5 min using the 500 W white light source in a fixed distance of 40 cm. Alternatively, singlet oxygen was generated by chemiexcitation via thermodecomposition of the endoperoxide NDPO2.12,32
Experimental design
All measurements were performed with cells from passages 2–8. Endothelial cells were cultured in 12-well tissue culture plates (2×105) or on 8-well chamber-Tec glass slides (1×104) in a humidified incubator at 37°C in RPMI 1640/ 20% FCS. Endothelial apoptosis was induced by irradiation with UVA1 (2–10 J/cm2) or H2O2 challenge (0.1–0.9 mM) whereas necrosis was achieved by singlet oxygen generated from Rose Bengal at the concentrations indicated plus light-treatment (RB/hν). During or at indicated time points after UVA1 irradiation, RB/hν challenge or hydrogen peroxide incubation resident endothelial cells were incubated with the respective additives at concentrations indicated and 24 h after irradiation the relative number of living endothelial cells was detected by neutral red staining as described previously.10 Additionally, viability of endothelial cells was routinely controlled at the beginning and the end of every experiment using the trypan blue exclusion assay or propidium iodide staining. Viable cells were defined as cells excluding trypan blue or propidium iodide and positive for respiratory activity as determined by neutral red.
Detection of apoptotic or necrotic cells
At different time points (1–24 h) after UVA1-irradiation (2–10 J/cm2), RB/hν-challenge or H2O2 incubation endothelial cells grown in 12-well culture plates were washed with PBS, stained with Hoechst dye H33342 (8 μg/ml) and/or propidium iodide (0.5 μg/ml) for 5 min and nuclei or necrotic cells were visualized using a Zeiss fluorescence microscope, respectively. In each sample a minimum of 400 cells was counted and condensed or fragmented nuclei as well as necrotic cells were expressed as per cent of total cells.
Detection and quantification of nuclear DNA fragmentation
DNA strand breaks of cells grown on 8-well chamber-tec slides were visualized by the in situ nick-translation method37 1–24 h after UVA-irradiation (2–10 J/cm2). In acetone fixed cells endogenous peroxidase activity was blocked with methanol+0.3% H2O2 for 30 min. The nick-translation mixture contained 3 μM biotin-dUTP, 5 U/100 μl Kornberg polymerase, 3 μM each dGTP, dATP, dCTP, 50 mM Tris-HCL, pH 7.5, 5 mM MgCl2, 0.1 mM dithiothreitol, and reaction was performed at room temperature for 20 min. Slides were washed in PBS and processed for immunocytochemical detection of biotin-labeled UTP by peroxidase-labeled avidin, followed by an enzyme reaction using DAB as substrate. In each sample a minimum of 500 cells were counted and labeled nuclei were expressed as per cent of total nuclei.
Use of antioxidants
For examining the role of reactive oxygen species (ROS) in cytotoxicity during or at time points indicated after UVA1-irradiation, RB/hν challenge or H2O2 incubation, endothelial cells were incubated with inhibitors of the respective ROS class.
Inhibition of singlet oxygen (1O2) action was achieved by addition of sodium azide (20 mM), histidine (40 mM), or imidazole (40 mM). In contrast, increasing of 1O2 half-life and thus its action was achieved in the presence of deuterated water (D2O, 99% atom).38,39,40 These agents were added to the cells 10 min prior to, were present during, and for 5 min after the respective procedure (10/present/5). To deplete superoxide anions (O2.−) SOD (1000 U/ml; 60/present/5) but also the O2.− quencher MnTBAP (80 μM; 0/absent/30) or MnTMPyP (150 μM; 0/absent/30) 41,42 were used. As a control, heat-inactivated SOD (10 min at 100°C) was used, and to inhibit the cytosolic Cu/Zn SOD the powerful inhibitor diethyldithiocarbamate (1 mM; 30/present/5) was used.43 Hydrogen peroxide (H2O2) was degraded by catalase (2000 U/ml; 60/absent/5), and as a control, heat-inactivated catalase (20 min at 100°C) was used, and intracellular catalase activity was inhibited using 3-amino-1,2,4-triazole (500 μM; 30/present/5).44 Inhibition of lipid peroxide formation was achieved with BHT (10 μM; 30/present/5),45 and for hydroxyl radical (OH.) quenching DMSO (100 mM; 30/present/5) or mannitol (100 mM; 30/present/5) were used.46,47 In experiments examining H2O2 toxicity the respective agents (1 mM DETA/NO, 1 mM DETA, 4000 U/ml catalase, heat-inactivated catalase) were added 10 min prior to the addition of hydrogen peroxide and were present during the 24 h of incubation.
In experiments examining the time-course of ROS action the respective agents were added for 30 min to the cell cultures at the different time points indicated after the toxic insult. In the case of incubation with H2O2 the respective agents (1 mM DETA/NO, 1 mM DETA, 4000 U/ml catalase, heat-inactivated catalase) were added to the cell cultures for 30 min after 90 min of incubation with 0.4, 0.7 or 0.9 mM H2O2, then cell cultures were washed twice with PBS and grown in culture medium for 24 h. At the concentrations used, none of the compounds mentioned above showed any cytotoxic effects towards the EC within the incubation time.
Detection of intracellular H2O2
Intracellular H2O2 formation was visualized using the fluorescent dye dihydrorhodamine 123 (DHR). Endothelial cells (1×105) in 12 well tissue culture plates were loaded with DHR (10 μM) for 45 min and washed with PBS before treatment with UVA1 or RB/hν. During the intracellular release of H2O2, reduced DHR is irreversibly oxidized and converted to the fluorescent compound rhodamine 123.48 Between 20 and 120 min after UVA1-irradiation rhodamine 123 formation was constant and was visualized using a Zeiss fluorescence microscope.
Detection of lipid peroxidation in UVA1-irradiated endothelial cells and measurement of microsomal lipid peroxidation
Resting endothelial cells (1×106) in 6-well tissue culture plates were irradiated with UVA1 (8 J/cm2), were exposed to RB/hν (1.5 μM) or incubated with H2O2 (0.9 mM) in the absence or presence of the respective additives at the concentrations indicated. One hundred and twenty or 60 min after irradiation lipid peroxidation was stopped by addition of BHT (10 μM), respectively. Cells were harvested and lysed by repeated freezing and thawing. Malonedialdehyde (MDA) equivalents were estimated via the formation of thiobarbituric acid (TBA)-reactive substances using ε535=156 mM−1cm−1.49
Additionally, in a cell-free system lipid peroxidation was initiated in liposomes (0.5 mg protein/ml) by singlet oxygen generated by thermal decomposition from NDPO2 (20 mM) with premixed ADP (1 mM)/FeCl3 (10 μM), and NADPH regenerating system, containing NADPH (0.4 mM), glucose-6-phosphate (10 mM), glucose-6-phosphate dehydrogenase (5 units/ml)50 in the presence or absence of the NO donor MAHMA/NO (5 mM; 1–2 min half-life for NO release at 37°C), denitrosylated MAHMA/NO (MAHMA, 5 mM), sodium azide (20 mM) or NDP (20 mM) alone. Lipid peroxidation was assayed as described above.
Western-blot analysis
Resting or UVA1-irradiated (8 J/cm2) endothelial cells (4×107), irradiated in the presence or absence of the compounds indicated, were detached after an incubation time of 1, 2 or 4 h by trypsin treatment, and washed twice with ice-cold PBS. The cell pellets were suspended in three volumes of ice-cold isolation buffer (0.25 M saccharose, 10 mM triethanolamine/HCl, 5 mM KH2PO4, 20 mM KCl, 2 mM EDTA, 5 mM MgCl2, pH 7.0) supplemented with the protease inhibitor mix from Boehringer. After 15 min on ice, the cells were disrupted by douncing in a 2 ml glass douncer. Intact cells and nuclei were separated from cytosolic fraction by two centrifugation steps (10 min at 2000 × g and 25 min at 16 500 × g). Pellets or mitochondria-free supernatants were mixed with the sample buffer (Novex, San Diego, CA, USA). Proteins (50 μg per lane taken from the pellet fraction for Bcl-2 or Bax determination or 100 μg per lane taken from the mitochondria-free supernatant for holocytochrome c determination) were separated by electrophoresis in a gradient (4–12%) bis-tris-polyacrylamide gel with MOPS-SDS running buffer (Novex) and transferred to nitrocellulose membranes. Further incubations of the blots were: 1 h with blocking buffer (2% BSA, 5% non-fat milk powder, 0.1% Tween 20 in PBS-buffer), 1 h with a 1 : 1000 dilution of the monoclonal mouse anti-holocytochrome c antibody or the rabbit anti-Bcl-2 or rabbit anti-Bax antiserum, washed, 1 h with a 1 : 1000 dilution of the secondary horseradish peroxidase conjugated goat anti-mouse IgG antibody or horseradish peroxidase conjugated porcine anti-rabbit IgG antibody. Finally, blots were incubated for 5 min in ECL reagent (Pierce, Rockford, IL, USA), placed into a plastic bag and exposed to an enhanced autoradiographic film. To control equal loading of total protein in all lanes, blots were stained with a 1 : 2000 solution of the mouse anti α-tubulin antibody. The secondary horseradish peroxidase conjugated goat anti-mouse IgG antibody was diluted 1 : 2000 prior to use.
Statistical analysis
Data are given as means±S.D. Values were calculated using analysis with Student's t-test (two-tailed for independent samples).
Abbreviations
- BHT:
-
butylated hydroxytoluene
- EC:
-
endothelial cells
- iNOS:
-
inducible nitric oxide synthase
- NO:
-
nitric oxide
- RB/hν:
-
Rose Bengal plus visible light
- ROS:
-
reactive oxygen species
- SNOC:
-
S-nitrosocysteine
- SOD:
-
superoxide dismutase
- UVA1:
-
ultraviolet radiation A1
References
Passchier WF, Bosnjakovic BFM . 1987 Human Exposure to Ultraviolet Radiation. Amsterdam
Webb RB . 1977 Lethal and mutagenic effects of near-ultraviolet radiation. In Photochemistry and Photobiology Reviews. Smith KC, ed New York: Plenum pp. 169–262
Tyrrell RM, Keyse SM . 1990 The interaction of UVA radiation with cultured cells J. Photochem. Photobiol. 4B: 349–361
Black HS . 1987 Potential involvement of free radical reactions in ultraviolet light-mediated cutaneous damage Photochem. Photobiol. 46: 213–221
Adams JM, Cory S . 1998 The Bcl-2 protein family: arbiters of cell survival Science 281: 1322–1326
Kim Y-M, Bombeck CA, Billiar TR . 1999 Nitric oxide as a bifunctional regulator of apoptosis Circ. Res. 84: 253–256
Förstermann U, Closs EI, Pollock JS, Nakane M, Schwarz P, Gath I, Kleinert H . 1994 Nitric oxide synthase isoenzymes. Characterisation, purification, molecular cloning, and functions Hypertension 23: 1121–1131
Kröncke K-D, Fehsel K, Kolb-Bachofen V . 1995 Inducible nitric oxide synthase and its product nitric oxide, a small molecule with complex biological activities Biol. Chem. 376: 327–343
Suschek C, Rothe H, Fehsel K, Enczmann J, Kolb-Bachofen V . 1993 Induction of a macrophage-like nitric oxide synthase in cultured rat aortic endothelial cells J. Immunol. 151: 3283–3291
Suschek CV, Krischel V, Bruch-Gerharz D, Berendji D, Krutmann J, Kröncke K-D, Kolb-Bachofen V . 1999 Nitric oxide fully protects against UVA-induced apoptosis in tight correlation with Bcl-2 up-regulation J. Biol. Chem. 274: 6130–6137
Klotz L-O, Pellieux C, Briviba K, Pierlot C, Aubry J-M, Sies H . 1999 Mitogen-activated protein kinase (p38, JNK-, ERK-) activation pattern induced by extracellular and intracellular singlet oxygen and UVA Eur. J. Biochem. 260: 917–922
Briviba K, Klotz L-O, Sies H . 1997 Toxic and signaling effects of photochemically or chemically generated singlet oxygen in biological systems Biol. Chem. 378: 1259–1265
Tyrrell RM, Pidoux M . 1989 Singlet oxygen involvement in the inactivation of cultured human fibroblasts by UVA (334 nm, 365 nm) and near-visible (405 nm) radiation Photochem. Photobiol. 49: 407–412
Crow JP . 1997 Dichlorodihydrofluorescein and dihydrorhodamine 123 are sensitive indicators of peroxynitrite in vitro: implications for intracellular measurement of reactive nitrogen and oxygen species Nitric Oxide 1: 145–157
Danpure HJ, Tyrrell RM . 1976 Oxygen dependence of near-UV (365 nm) lethality and the interaction of near-UV and X-rays in two mammalian cell lines Photochem. Photobiol. 23: 171–177
McCormick JP, Fischer JR, Pachlatko JP . 1976 Characterization of a cell-lethal product from the photooxidation of tryptophan: hydrogen peroxide Science 191: 468–469
Czochralska B, Kamczynski W, Bartosz G, Shugar D . 1984 Oxidation of excited-state NADH and NAD dimer in aqueous medium involvement of O2− as a mediator in the presence of oxygen Biochim. Biophys. Acta. 801: 403–409
Peak JG, Peak MJ, Foote CS . 1982 Effects of glycerol upon the biological action of near-ultraviolet light: spectra and concentration dependence for transforming DNA and for Escherichia coli B/r Photochem. Photobiol. 3: 413–416
Kanofsky JR . 1989 Singlet oxygen production by biological systems Chem-Biol. Interact. 70: 1–28
Janssen YMW, Van Houten B, Borm PJA, Mossman BT . 1993 Biology of Disease: cell and tissue responses to oxidative damage Lab. Invest. 69: 261–274
Sies H . 1986 Biochemistry of oxidative stress Angew. Chem. Int. Ed. 25: 1058–1071
Ramakrishnan N, McClain DE, Catravas GN . 1993 Membranes as sensitive targets in thymocyte apoptosis Int. J. Radiat. Biol. 63: 693–701
Forrest VJ, Kang Y-H, McClain DE . 1994 Oxidative stress-induced apoptosis prevented by Trolox Free Radical Biol. Med. 16: 675–684
Kuhn A, Fehsel K, Lehmann P, Krutmann J, Ruzicka T, Kolb-Bachofen V . 1998 Aberrant timing in epidermal expression of inducible nitric oxide synthase after UV-irradiation in Lupus patients J. Invest. Dermatol. 111: 149–153
Leist M, Single B, Castoldi AF, Kühnle P, Nicotera P . 1997 Intracellular adenosine triphosphate (ATP) concentrations: A switch in the decision between apoptosis and necrosis J. Exp. Med. 185: 1481–1486
Kröncke K-D, Fehsel K, Kolb-Bachofen V . 1997 Nitric oxide: cytotoxicity versus cytoprotection: How, why, when, and where? Nitric Oxide Biol. Chem. 1: 107–120
Ryter SW, Tyrrell RM . 1998 Singlet molecular oxygen ((1)O2): a possible effector of eukaryotic gene expression Free Radic Biol. Med. 24: 1520–1534
McCaughan Jr JS . 1999 Photodynamic therapy: a review Drugs Aging 15: 49–68
Fukuto JM, Cho JY, Switzer CH . 2000 The chemical properties of nitric oxide and related nitrogen oxides. In: Nitric Oxide: Biology and Pathobiology. Ignarro LJ, ed San Diego: Academic Press pp. 23–40
Darley-Usmar VM, Patel RP, O'Donnell VB, Freeman BA . 2000 Antioxidant actions of nitric oxide. In: Nitric Oxide: Biology and Pathobiology. Ignarro LJ, ed San Diego: Academic Press pp. 265–276
Miranda KM, Espey MG, Jourd'heuil D, Grisham MB, Fukuto J, Feelisch M, Wink DA . 2000 The chemical biology of nitric oxide. In: Nitric Oxide: Biology and Pathobiology. Ignarro LJ, ed San Diego: Academic Press pp. 41–56
Di Mascio P, Sies H . 1989 Quantification of singlet oxygen generated by thermolysis of 3,3′-(1,4-naphthylidene)dipropionate. Monomol and dimol photoemission and the effects of 1,4-diazabicyclo [2.2.2] octane J. Am. Chem. Soc. 111: 2909–2914
Kröncke K-D, Kolb-Bachofen V . 1996 Detection of nitric oxide interaction with zinc finger proteins Meth. Enzymol. 269: 279–284
Hrabie JA, Klose JR, Wink DA, Keefer LK . 1993 New nitric oxide-releasing zwitterions derived from polyamines J. Org. Chem. 58: 1472–1476
Suschek C, Fehsel K, Kröncke K-D, Sommer A, Kolb-Bachofen V . 1994 Primary cultures of rat capillary endothelial cells: constitutive and cytokine-inducible macrophage-like nitric oxide synthases are expressed and activities regulated by glucose concentration Am. J. Pathol. 145: 485–695
Klotz L-O, Briviba K, Sies H . 1997 Singlet oxygen mediates the activation of JNK by UVA radiation in human skin fibroblasts FEBS Lett. 408: 289–291
Fehsel K, Kolb-Bachofen V, Kolb H . 1991 Analysis of TNF-alpha-induced DNA strand breaks at the single cell level Am. J. Path. 139: 251–157
Kaiser S, DiMascio P, Murphy ME, Sies H . 1990 Physical and chemical scavenging of singlet molecular oxygen by tocopherols Arch. Biochem. Biophys. 277: 101–108
Egorov SY, Kurella EG, Boldyrev AA, Krasnovsky AAJ . 1997 Quenching of singlet molecular oxygen by carnosine and related antioxidants. Monitoring 1270-nm phosphorescence in aqueous media Biochem. Mol. Biol. Int. 41: 687–694
Michaeli A, Feitelson J . 1994 Reactivity of singlet oxygen toward amino acids and peptides Photochem. Photobiol. 59: 284–289
Faulkner KM, Stevens RD, Fridovich I . 1994 Characterization of Mn(III) complexes of linear and cyclic desferrioxamines as mimics of superoxide dismutase activity Arch. Biochem. Biophys. 310: 341–346
Faulkner KM, Liochev SI, Fridovich I . 1994 Stable Mn(III) porphyrins mimic superoxide dismutase in vitro and substitute for it in vivo J. Biol. Chem. 269: 23471–23476
Heikkila RE, Cabbat FS, Cohen G . 1976 In vivo inhibition of superoxide dismutase in mice by diethyldithiocarbamate J. Biol. Chem. 251: 2182–2185
Williams RN, Delamere NA, Paterson CA . 1985 Inactivation of catalase with 3-amino-1,2,4-triazole: an indirect irreversible mechanism Biochem. Pharmacol. 34: 3386–3389
Bose B, Agarwal S, Chatterjee SN . 1989 UV-A induced lipid peroxidation in liposomal membrane Radiat. Environ. Biophys. 28: 59–65
Babbs CF, Griffin DW . 1989 Scatchard analysis of methane sulfinic acid production from dimethyl sulfoxide: a method to quantify hydroxyl radical formation in physiologic systems Free Radic. Biol. Med. 6: 493–503
Chaturvedi V, Wong B, Newman SL . 1996 Oxidative killing of Cryptococcus neoformans by human neutrophils. Evidence that fungal mannitol protects by scavenging reactive oxygen intermediates J. Immunol. 156: 3836–3840
Royall JA, Ischiropoulos H . 1993 Evaluation of 2′,7′-dihydrofluorescin and dihydrorhodamine 123 as fluorescent probes for intracellular H2O2 in cultured endothelial cells Arch. Biochem. Biophys. 302: 348–355
Knight JA, Pieper RK, McClellan L . 1988 Specificity of the thiobarbituric acid reaction: its use in studies of lipid peroxidation Clin. Chem. 34: 2433–2438
Scheschonka A, Murphy ME, Sies H . 1990 Temporal relationships between the loss of vitamin E, protein sulfhydryls and lipid peroxidation in microsomes challenged with different prooxidants Chem-Biol Interact. 74: 233–252
Acknowledgements
We thank Christa-Maria Wilkens-Roth, Annette Reimann, Marija Lenzen, and Ulla Lammersen for technical assistance, and Martha Turken for photographic assistance. This study was supported by grants from the Deutsche Forschungsgemeinschaft (SFB 503, A3 and B1) and by NFCR.
Author information
Authors and Affiliations
Corresponding author
Additional information
Edited by A Finazzi-Agro
Rights and permissions
About this article
Cite this article
Suschek, C., Briviba, K., Bruch-Gerharz, D. et al. Even after UVA-exposure will nitric oxide protect cells from reactive oxygen intermediate-mediated apoptosis and necrosis. Cell Death Differ 8, 515–527 (2001). https://doi.org/10.1038/sj.cdd.4400839
Received:
Revised:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1038/sj.cdd.4400839
Keywords
This article is cited by
-
Receptor interacting protein 3 kinase, not 1 kinase, through MLKL-mediated necroptosis is involved in UVA-induced corneal endothelium cell death
Cell Death Discovery (2021)
-
Corneal endothelial loss after crosslinking with riboflavin and ultraviolet-A
Graefe's Archive for Clinical and Experimental Ophthalmology (2012)
-
Photolytically generated nitric oxide inhibits caspase activity and results in AIF-mediated cell death
Journal of Molecular Medicine (2010)
-
Topically Applied Nitric Oxide Induces T-Lymphocyte Infiltration in Human Skin, but Minimal Inflammation
Journal of Investigative Dermatology (2008)
-
Evidence for Hydroxyl Radical Scavenging Action of Nitric Oxide Donors in the Protection Against 1-Methyl-4-phenylpyridinium-induced Neurotoxicity in Rats
Neurochemical Research (2008)