Mitogen-activated protein kinase activation by oxidative and bacterial stress in an amphibian cell culture model. (Research Articles).
Amphibians are particularly sensitive to environmental stress due to their unique life-history strategies that lead to their exposure to natural and anthropogenic perturbations in both aquatic and terrestrial ecosystems. Because amphibians have thin, permeable skin and their eggs lack shells, they are susceptible to environmental exposure during development and as adults. Therefore, they may serve as important sentinel species to changes in environmental conditions. Since the mid-1990s, unusually large numbers of frogs with malformations have been found in North America (1,2). Abnormalities have been reported in 36 species of amphibians from 42 U.S. states. There is also concern that the environmental factors causing these anuran deformities may affect human health. The reason for the amphibian malformations and population decline remains unknown, although it has been suggested that parasitic infections, UV radiation, and chemical pollutants could play a role (3). If endoparasitic infestations are involved, it is likely that environmental stress (i.e., UV radiation, pollution) could increase susceptibility to these infections (4). It is also reasonable to assume that a number of critical environmental interactions could contribute to the detrimental effects on amphibian populations (5,6).
There has also been a rapid decline and range reduction of certain amphibian species worldwide over the past two decades. However, some species within the same regions do not appear to be affected, whereas others are driven to extinction (7). Although the explanation for the degradation of amphibian populations is currently disputed, Pechmann et al. (8) caution that it may be difficult to distinguish natural population fluctuations from human-induced declines without long-term surveys at numerous sites to isolate the various confounding components. However, anthropogenic factors such as water pollution and atmospheric conditions such as ozone depletion and/or UV radiation could play important roles (4,6). Continuing population reductions and morphologic defects in anurans has generated international interest. A primary consideration in the correlation of this problem to human health is our dependence on water quality. Therefore, frogs are an important sentinel species that may indicate environmental deterioration. Although there has been much investigation into the causal factors contributing to malformations and declining amphibian numbers, in vitro cell culture models to address which environmental pollutants cause cellular stress in amphibians are lacking.
A major indicator of cellular stress is the activation of a class of intracellular proteins called mitogen-activated protein (MAP) kinases, which are a family of serine/threonine kinases that include extracellular signal-regulated kinases (ERKs), p38 MAP kinases, and c-jun N-terminal kinases (JNKs) (9). MAP kinases normally regulate a variety of cellular activities in response to endogenous cytokines and growth factors, leading to biologic outcomes such as cell growth and differentiation (10). Several environmental agents activate MAP kinases to cause cellular stress and cytotoxic responses, including bacterial products (such as lipopolysaccharide; LPS), pesticides, certain transition metals, and UV radiation (11-13). Transition metals and UV radiation cause MAP kinase activation via the generation of reactive oxygen species (14,15). In particular, UV radiation has been implicated as a major factor in amphibian mortality and deformities (16-19).
In this study, we investigated MAP kinase (ERK) activation in Senopus tadpole cells (XTC-2). The XTC-2 cells were treated with a reactive oxygen species (hydrogen peroxide; [H.sub.2][O.sub.2]) or a bacterial wall product, LPS. Both of these factors are associated with environmental stress in polluted aquatic ecosystems (20,21). [H.sub.2][O.sub.2] and LPS both caused phosphorylation of ERK-2 in XTC-2 cells in a time- and dose-dependent manner. These data suggest that the ERK-2 pathway is a senstitive biomarker to detect environmental stress and that the ERK pathway mediates cell death in response to [H.sub.2][O.sub.2] and LPS.
Materials and Methods
Materials. Goat polyclonal anti-ERK-1/2 (catalog no. SC-154-G) that recognizes total cellular ERK (i.e., both phosphorylated and unphosphorylated forms) was purchased from Santa Cruz Biotechnology (Santa Cruz, CA). This antibody was raised against an epitope mapping the carboxy terminus of ERK-2-encoded MAP kinase p42 of rat origin. The antibody is reactive with ERK-2 and to a lesser extent ERK-1 and possesses broad interspecies reactivity (murine, human, chicken, and frog). To verify that we were detecting only ERK-2 and not ERK-1 in XTC-2 cells, we used two other antibodies raised against total ERK-1 and -2 from Transduction Laboratories (Lexington, KY) or Upstate Biotechnologies (Lake Placid, NY). An anti-phospho-ERK-1/2 monoclonal antibody that is specific for the phosphorylated forms of ERK-1/2 (catalog no. 9106) was purchased from Cell Signaling Technologies/New England Biolabs (Beverly, MA). This antibody had previously been reported by the company to cross-react with ERK-1/2 from human, rat, mouse, and hamster (no information on Xenopus was available). Anti-mouse IgG-HRP was purchased from Transduction Laboratories, and anti-goat IgG-HRP was purchased from DakoPatts (Carpenteria, CA). E. coli LPS (no. L8274) and [H.sub.2][O.sub.2] were purchased from Sigma Chemical Company (St. Louis, MO). The MEK/ERK inhibitor, PD98059, was purchased from Calbiochem (La Jolla, CA).
Cell culture. Xenopus tadpole cells (XTC-2) were kindly provided by P. Blackshear at NIEHS and were originally obtained from D. J. Shapiro at the University of Illinois-Urbana (22). Aliquots of XTC-2 thawed from liquid nitrogen storage were seeded in culture flasks containing Leibovitz's L-15 medium supplemented with 10% fetal bovine serum (Sigma). Cultures of XTC-2 were grown in 175 [cm.sup.2] sterile, plastic culture flasks at room temperature with humidified air. At confluence, the cells were liberated from the culture surface with a 1:10 dilution of trypsin (Gibco, Grand Island, NY) in 1 mM EDTA/phosphate-buffered saline, pH 7.4. Cells were then plated in 75-[cm.sup.2] plastic culture dishes, grown to confluence, and growth arrested in serum-free Leibovitz's L-15 medium for 24 hr before treatment with [H.sub.2][O.sub.2] or LPS.
Western blotting. After treating XTC-2 cells with [H.sub.2][O.sub.2] or LPS, the cells were placed on ice and washed twice with ice-cold phosphate-buffered saline (PBS), and after all the residual PBS was carefully removed, 100 [micro] L of lysis buffer was added to the cell monolayer. The lysis buffer consisted of 50 mM HEPES, 150 mM NaCl, 1% Triton X-100, 1 mM PMSF, and 20 [micro] g/mL aprotinin, leupeptin, and pepstatin. The cellular protein was then removed from the culture surface with a cell scraper and lysates were clarified by centrifugation at 13,000 rpm for 10 min and frozen at -80[degrees]C. We loaded 20 [micro] g of protein from each sample on an 8-16% SDS-PAGE gel. Separated proteins were then transferred to a nitrocellulose membrane, and the membrane was blocked for 2 hr at room temperature with 5% nonfat milk in Tris-buffered saline-Tween buffer (20 mM Tris, 500 mM NaCl, 0.01% Tween 20). The membrane was then incubated with the anti-phospho-ERK-1/2 antibody (1:1,000 dilution) at 4[degrees]C overnight, followed by incubation for 2 hr with a 1:2,000 dilution of horseradish peroxidase-conjugated anti-mouse IgG. The immunoblot was visualized through enhanced chemiluminescence (Amersham, Arlington Heights, ID. The same blot was subsequently stripped at 50[degrees]C for 30 min in a buffer containing 62.5 mM Tris (pH 6.7), 2% SDS, and 100 mM 2-mercaptoethanol. The stripped blots were incubated with polyclonal anti-ERK-1/2 (1:1,000 dilution) at 4[degrees]C overnight, followed by incubation for 2 hr with a 1:2,000 dilution of horseradish peroxidase-conjugated antigoat IgG.
Cytotoxicity assay. We measured cytotoxicity by the tetrazolium salt (MTT) cell viability assay according to the manufacturer's instructions (Boehringer Mannheim, Indianapolis, IN). Absorbance was measured at 570 nm with a 630 nm reference filter. The negative control was the absorbance of cells with medium alone. The postive control (100% cytotoxicity) was determined by treating cells with distilled water for 24 hr.
Densitometric evaluation of ERK activation and statistical analysis. Autoradiographic images from the Western blots were digitally scanned and densitometric measurements for phospho-ERK and total ERK signals were performed using the NIH Image program. The phospho-ERK signal was normalized against the corresponding total ERK signal from the same Western blot to obtain the phospho-ERK/ERK ratio. In all experiments, Western blotting was performed first for phospho-ERK (Cell Signaling, catalog no. 9106), then the blots were stripped and reblotted for total ERK using an antibody that recognizes the total ERK (Santa Cruz, catalog no. SC-154-G). The data were expressed as fold-increase over control (i.e., cells treated with medium alone). We repeated each experiment at least three times and determined significant differences by one-way analysis of variance (ANOVA). For cytotoxicity data, we analyzed comparisons of control versus treatment by paired t-tests.
XTC-2 cells contain ERK-2. We investigated MAP kinase activation in confluent, quiescent cultures of Xenopus (XTC-2) cells as an in vitro model of oxidant- and bacterial-induced cellular stress. We first determined whether XTC-2 cells possessed either the p42 (ERK2) or p44 (ERK-1) isozymes of MAP kinase. We detected only ERK-2 (p42 MAP kinase) in XTC-2 cells, whereas both ERK-1 and ERK-2 were readily detectable in human lung fibroblasts (Figure 1). Similar results were obtained using two other polydonal antibodies raised against total ERK-1 and ERK-2 (data not shown). Therefore, although we cannot rule out that XTC-2 cells might possess ERK-1, we clearly demonstrated that our assay detects only ERK-2.
[FIGURE 1 OMITTED]
Rapid activation of ERK-2 by oxidative strew. We next evaluated whether oxidative stress would activate ERK-2 in XTC-2 cells, as has been reported in mammalian cell culture systems (23). ERK-2 phosphorylation peaked 30 min after [H.sub.2][O.sub.2] treatment, causing a 25-fold increase in the phospho-ERK-2/ERK-2 ratio, and gradually declined over 2 hr. One-way ANOVA for the [H.sub.2][O.sub.2] time course yielded a calculated F value of 3.12 (p = 0.049; Figure 2). The 30-min time point was used for further experiments evaluating the concentration-dependent activation of ERK-2. [H.sub.2][O.sub.2]-induced ERK-2 activation was maximal at 10 [micro] M [H.sub.2][O.sub.2] and did not significantly increase further at 50 [micro] m [H.sub.2][O.sub.2] (Figure 3). One-way ANOVA for the [H.sub.2][O.sub.2] dose response yielded a calculated F value of 3.85 (p = 0.038). In all of these experiments, the signal for total ERK-2 protein did not change with [H.sub.2][O.sub.2] treatment.
[FIGURES 2-3 OMITTED]
Delayed activation of ERK-2 by LPS. We then investigated whether ERK-2 in XTC-2 cells was a target for endotoxin-mediated cell stress. ERK-2 phosphorylation peaked 60 min after LPS treatment, causing a 5- to 10-fold increase in the phospo-ERK-2/ERK-2 ratio (Figure 4). These data indicated that LPS was a weaker activator of ERK-2 compared to [H.sub.2][O.sub.2], and the ERK-2 phosphorylation response to LPS was delayed by as much as 30 min compared to [H.sub.2][O.sub.2]. LPS caused a concentration-dependent increase in ERK-2 activation that was maximal at 50-500 [micro] g/mL LPS (Figure 5). One-way ANOVA yielded a calculated F value of 2.57 (p = 0.08) for the LPS time-course data (Figure 4) and of 2.80 (p = 0.08) for dose response (Figure 5).
[FIGURES 4-5 OMITTED]
Effect of ERK inhibition on [H.sub.2][O.sub.2]- and LPS-induced cytotoxicity. [H.sub.2][O.sub.2] and LPS both caused a concentration-dependent increase in cytotoxiciry after 24 hr as determined by MTT assay (Figure 6). Parallel cultures of cells in log-phase growth (i.e., cells exposed in medium containing 10% fetal bovine serum) were pretreated with either 50 [micro] m PD98059 (MEK/ERK inhibitor) or dimethylsulfoxide vehicle control for 1 hr before treatment with [H.sub.2][O.sub.2] or LPS. Pretreatment of XTC-2 cells with PD98059 significantly reduced the cytotoxic response to either [H.sub.2][O.sub.2] or LPS (Figure 6). Marginal cytotoxicity was observed in quiescent cultures of XTC-2 cells treated with [H.sub.2][O.sub.2] or LPS, indicating that co-stimulation of cells with growth-stimulatory factors in serum plus the environmental stressor ([H.sub.2][O.sub.2] or LPS) were required for a maximal cytotoxic response. These data indicated that the cytotoxic effects of reactive oxygen species or bacterial endotoxin are mediated at least in part through activation of the ERK pathway. Significant differences between control versus treatment with PD98059 were determined by paired t-tests.
[FIGURE 6 OMITTED]
In this study, we found that the ERK-2 MAP kinase pathway in Xenopus (XTC-2) cells is activated by oxidative stress ([H.sub.2][O.sub.2]) or bacterial lipopolysaccharide (LPS). Moreover, ERK activation mediated, at least in part, the cytotoxic response to either [H.sub.2][O.sub.2] or LPS. This in vitro model of MAP kinase activation could help identify pollutants in aquatic ecosystems that contribute to the problem of amphibian malformations and population decline. Amphibians have evolved strategies to cope with harsh changes in natural conditions, including dessication of temporary water sources (24). Despite this resilience in the face of natural environmental changes, amphibians may be particularly susceptible to a wide range of environmental toxicants that are present in polluted waters. The XTC-2 cell culture model might be useful for detecting cellular stress induced by pollutants that generate reactive oxygen species (e.g., metals, pesticides) or gram-negative bacteria that release endotoxin.
The XTC-2 in vitro model for measuring ERK-2 activation could also be used to test the effects of UV radiation generated in the laboratory. UV radiation has been proposed as a major stress factor for some amphibian populations (4,16,19). Moreover, it is important to consider that UV radiation may alter the chemical structure of some xenobiotics and thereby enhance toxicity. For example, Zaga and colleagues (25) reported that UV radiation enhanced the toxicity of carbaryl (a broad spectrum insecticide) to Xenopus laevis and Hyla versicolor embryos and tadpoles. Therefore, future investigation should include studies on agents such as carbaryl that are photoactivated by UV radiation to determine if this enhances the cellular stress response (e.g., ERK-2 activation) in cultured Xenopus cells.
The activation of MAP kinase signaling pathways in response to endogenous growth factors is well established and produces cell growth or differentiation (26,27). A variety of polypeptide growth factors (e.g., fibroblast growth factor-2 (FGF), platelet-derived growth factor (PDGF), epidermal growth factor (EGF) bind to specific cell-surface receptors and initiate an intracellular signal transduction cascade involving the sequential phosphorylation of Ras, Raf, Map kinase kinase (MEK), and ERK. ERK then translocates to the nucleus, where it phosphorylates a variety of transcription factors that control gene expression (9). Xenopus oocyte maturation requires phosphorylation and activation of p42 MAP kinase, and the corresponding dephosphorylation and inactivation of the enzyme is crucial for the transition of the zygote from meiosis through the first phases of mitosis (10). Likewise, Bitangcol et al. (28) found that p42 MAP kinase activation regulates the normal progression through the cell cycle and is an essential component of the spindle assembly checkpoint. Furthermore, during Xenopus development, ordinary mesoderm differentiation relies on MAP kinase activation in response to FGF. However, overexpression of Xenopus MAP kinase phosphatase obstructs mesoderm induction by FGF and produces characteristic defects in mesoderm formation in intact embryos (29). We postulate that oxidative or bacterial stress that activates the ERK-2 pathway during development could contribute to the morphologic anomalies seen in frogs, especially those involving mesodermal derivatives such as bone and muscle differentiation in the limbs. In fact, our cytotoxicity data showed that [H.sub.2][O.sub.2] or LPS caused more toxicity when cells were exposed in log-phase growth (i.e., in the presence of medium containing 10% fetal bovine serum) compared to cells in a quiescent state (Figure 6). Cells undergoing mitosis appear to be more susceptible to environmental stress.
Although the ERK-2 pathway is essential for growth and development mediated by growth factors, increasing evidence suggests that the ERK pathway is the target of environmental stress. Several environmental stressors (oxidants, metals, or UV radiation) cause ERK activation by first causing phosphorylation of the intracellular domain of the EGF receptor in a ligand-independent manner (i.e., in the absence of EGF) (9,15,30). ERK activation by these environmental agents generally causes cell death (apoptosis) rather than normal cell growth and differentiation. For example, [H.sub.2][O.sub.2] causes a cytotoxic response of mammalian connective tissue cells via the EGF receptor pathway leading to ERK activation, and a metabolic inhibitor of the ERK pathway (PD98059) blocked this cytotoxic response (23,30). We also observed that pretreatment of XTC-2 cells with PD98059 reduced the cytotoxic response of these cells to either [H.sub.2][O.sub.2] or LPS (Figure 6). Therefore, these environmental agents appear to cause XTC2 cell death in part via activation of ERK-2.
Our data show that both oxidative and bacterial stress trigger ERK phosphorylation in a time- and concentration-dependent manner. [H.sub.2][O.sub.2] caused a rapid and more pronounced phosphorylation of ERK-2, because maximal phosphorylation took place at 30 min (Figure 2) with a 20-fold increase from the control (Figure 3). In contrast, LPS was a weaker activator of ERK-2. The maximum phosphorylation response occurred after 60 min (Figure 4) with only a 5- to 10-fold increase from the control (Figure 5). These differences are likely due to different mechanisms of ERK activation by [H.sub.2][O.sub.2] and LPS. As mentioned above, [H.sub.2][O.sub.2] crosses the cell membrane and activates the intracellular domain of the EGF receptor, resulting in downstream activation of Ras, Raf, MEK, and ERK (30). In contrast, LPS docks to a cell-surface receptor, mCD14, which then complexes with a transmembrane signaling receptor, the toll-like receptor 4 (TLR4) (31). Activation of TLR4 then leads to ERK activation through a mechanism that is not yet clear (32). The different time-course response of ERK-2 to [H.sub.2][O.sub.2] in comparison to LPS could allow for discrimination of oxidative and bacterial stress in samples obtained from polluted waters.
Other types of pollution in aquatic systems should be considered as stress activators of MAP kinases. For example, metals may also represent a source of oxidative stress in polluted, aquatic environments (33). We have observed that vanadium pentoxide, a transition metal released from the industrial burning of fuel oil, causes ERK-2 activation in XTC-2 cells (data not shown). Also, pesticides have been associated with amphibian population declines (13). Certain pesticides recently have been reported to activate MAP kinase signaling pathways in a mammalian prostate cancer cell line (34). Therefore, it would be important to learn whether ERK-2 is activated by pesticides in the XTC-2 cell culture model.
In summary, we have shown that representative oxidative and bacterial agents cause activation of the ERK-2 MAP kinase in cultured Xenopus XTC-2 cells. [H.sub.2][O.sub.2] and LPS caused different temporal and dose-response patterns of ERK-2 activation. Blocking ERK-2 activation with the MEK inhibitor PD98059 partially protected XTC-2 cells against the cytotoxic effects of [H.sub.2][O.sub.2] or LPS. We propose that ERK-2 activation is a valuable biochemical marker for assessing factors that cause cellular stress in amphibians. Moreover, the XTC-2 cell culture model could be useful for rapidly assessing the "amphibian stress potential" of polluted waters. Future studies will address the utility of MAP kinase activation in XTC-2 cells as a screening assay for stressors present in the environment.
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Address correspondence to L. A. Bonnet, Pressly Building, Peace College, 15 East Peace Street, Raleigh, NC 27604 USA. Telephone: (919) 508-2266. Fax: (919) 508-2326. E-mail: firstname.lastname@example.org
We thank A. Rice at NIEHS for technical assistance and R. Wine at NIEHS for technical advice. We also thank J. Pritchard at NIEHS for useful suggestions during the preparation of the manuscript.
Received 10 October 2001; accepted 17 December 2001.
Lisa A. Carter, (1,2) Maija B. Tabor, (1,2) James C. Bonner, (2) and Lisa A. Bonner (1)
(1) Peace College, Raleigh, North Carolina, USA; (2) National Institute of Environmental Health Sciences, Research Triangle Park, North Carolina, USA
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|Author:||Bonner, Lisa A.|
|Publication:||Environmental Health Perspectives|
|Date:||Jul 1, 2002|
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