BioMed Research International

BioMed Research International / 2013 / Article
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Toxicology of Metals and Metalloids

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Research Article | Open Access

Volume 2013 |Article ID 769295 |

Tanara Vieira Peres, Daniela Zótico Pedro, Fabiano Mendes de Cordova, Mark William Lopes, Filipe Marques Gonçalves, Cláudia Beatriz Nedel Mendes-de-Aguiar, Roger Walz, Marcelo Farina, Michael Aschner, Rodrigo Bainy Leal, "In Vitro Manganese Exposure Disrupts MAPK Signaling Pathways in Striatal and Hippocampal Slices from Immature Rats", BioMed Research International, vol. 2013, Article ID 769295, 12 pages, 2013.

In Vitro Manganese Exposure Disrupts MAPK Signaling Pathways in Striatal and Hippocampal Slices from Immature Rats

Academic Editor: Wilma De Grava Kempinas
Received31 Jul 2013
Accepted07 Oct 2013
Published13 Nov 2013


The molecular mechanisms mediating manganese (Mn)-induced neurotoxicity, particularly in the immature central nervous system, have yet to be completely understood. In this study, we investigated whether mitogen-activated protein kinases (MAPKs) and tyrosine hydroxylase (TH) could represent potential targets of Mn in striatal and hippocampal slices obtained from immature rats (14 days old). The aim of this study was to evaluate if the MAPK pathways are modulated after subtoxic Mn exposure, which do not significantly affect cell viability. The concentrations of manganese chloride (MnCl2; 10–1,000 μM) caused no change in cell viability in slices exposed for 3 or 6 hours. However, Mn exposure significantly increased extracellular signal-regulated kinase (ERK) 1/2, as well as c-Jun N-terminal kinase (JNK) 1/2/3 phosphorylation at both 3 and 6 hours incubations, in both brain structures. Furthermore, Mn exposure did not change the total content or phosphorylation of TH at the serine 40 site in striatal slices. Thus, Mn at concentrations that do not disrupt cell viability causes activation of MAPKs (ERK1/2 and JNK1/2/3) in immature hippocampal and striatal slices. These findings suggest that altered intracellular MAPKs signaling pathways may represent an early event concerning the effects of Mn in the immature brain.

1. Introduction

Manganese (Mn) is an essential metal for humans and animals. Its essentiality is due to its requirement as a cofactor in chemical reactions catalyzed by several enzymes involved in cellular homeostasis, such as mitochondrial superoxide dismutase and glutamine synthetase. However, exposure to high Mn levels may cause a neurological syndrome referred to as manganism, which shares multiple analogous symptoms with Parkinson’s disease (PD) [1].

Within the central nervous system (CNS), Mn accumulates predominantly in structures of the basal ganglia, such as the striatum (caudate, putamen, and nucleus accumbens), globus pallidus, and substantia nigra, consistent with dystonia, bradykinesia and rigidity secondary to damage to dopaminergic neurons and gliosis [2, 3]. Nonmotor symptoms have also been reported in Mn-exposed individuals, such as loss of attention and neuropsychological symptoms, suggesting that not only the basal ganglia are affected in manganism [1, 4].

Neonatal and developing brains are more susceptible to Mn toxicity. The uptake of metal in the intestine is usually elevated in the first week of life, followed by a steady decrease with age. These factors contribute to the increased risk for neurotoxicity in newborns when exposed to excess Mn [5]. In addition, increased hair Mn levels (a useful analytical biomarker of Mn exposure in humans) has been associated with learning disabilities, hyperactivity, and attention deficit disorder [5]. In rats, exposure to Mn during development has been shown to affect the dopaminergic system and induce lasting motor impairment and astrocyte activation [6]. Nevertheless, despite evidence suggesting that precocious Mn exposure may impair neurological function later in life [6, 7], studies on the molecular targets of Mn during critical periods of brain development have yet to be systematically addressed.

Although the molecular mechanisms that mediate Mn-induced neurotoxicity have yet to be fully understood, evidence points to mitochondrial dysfunction with formation of reactive oxygen species (ROS) and oxidative stress as critical mediators of neurotoxicity [811]. Increased striatal levels of F2 isoprostanes as consequence of oxidative stress have been reported in response to Mn treatment in rats during development, with concomitant activation of the mitogen-activated protein kinase (MAPK) ERK1/2 [12, 13]. Of particular importance, studies in cell culture models have shown that Mn-induced oxidative stress is related, at least in part, to the activation of MAPK pathways [1417]. MAPKs are a family of serine-threonine kinases which play critical roles in neurodevelopment and neuroplasticity. They mediate various cellular responses, such as proliferation, differentiation, cell survival, death, and cell transformation. The three major MAPKs are extracellular signal-regulated kinases (ERK1/2), c-Jun N-terminal kinases (JNKs), and [18, 19].

Neurotransmission dyshomeostasis has been implicated in Mn neurotoxicity, and deregulated dopamine (DA) signaling has been a major focus of research (reviewed by Aschner et al. [1]). Due to similarities between manganism and PD and the accumulation of Mn in regions rich in dopaminergic (DAergic) neurons, altered DA metabolism has been considered an important aspect of the molecular actions of Mn [20]. Motor disturbances have been observed in children undergoing prolonged parenteral nutrition, where Mn is present at high concentrations [21]. In vitro evidence has shown that Mn decreases DA levels in the striatum due to direct oxidation of this monoamine [22]. Furthermore, Posser et al. [23] demonstrated that in PC12 cells low levels of Mn can induce sustained phosphorylation at serine (Ser) 40 of tyrosine hydroxylase (TH), the rate limiting enzyme for the synthesis of DA, leading to prolonged activation of the enzyme.

As noted above, activation of MAPK pathways has been linked to Mn-induced neurotoxicity [12, 14, 15, 17]. However, it is difficult to affirm whether MAPK activation is a cause or consequence of Mn-induced neurotoxicity. No reports were located to ascertain whether MAPK activation represents a primary event (that could trigger Mn toxicity) or if it occurs secondary to Mn-induced cellular dyshomeostasis/damage (triggered via other mechanisms, i.e., oxidative or metabolic changes). Accordingly, the aim of this study was to evaluate if MAPK pathways are modulated after Mn exposure when this metal is present at subtoxic concentrations, which are unable to change cell viability. In addition, the potential activation of TH was also investigated since it is important in maintaining homeostasis in DAergic neurons (targeted by Mn). To meet these objectives, fresh striatal and hippocampal slices from rats in a critical neurodevelopmental period (postnatal day 14/PND14) were acutely exposed to Mn (for 3–6 h). Our study indicates that disturbances in ERK and JNK activity in response to Mn may represent an early event. The occurrence of changes in ERK activity and JNK activity after Mn exposure, added to the absence of cell viability loss, suggests that the modulation of MAPK signaling pathway represents a primary event induced by Mn.

2. Methods

2.1. Chemicals

Anti-phospho-ERK1/2, anti-phospho-JNK1/2/3 antibodies, and LumiGLO chemiluminescent substrate were purchased from Cell Signaling (Beverly, MA, USA). Anti-phospho- , anti-total- , anti-total-ERK1/2, and anti-total-JNK1/2 antibodies and manganese chloride (MnCl2) and Dulbecco’s modified Eagle’s medium (DMEM) were obtained from Sigma (St. Louis, MO, USA). Anti-phospho-TH, anti-total-TH, and goat anti-rabbit IgG HRP (horseradish peroxidase) conjugate secondary antibodies were purchased from Millipore (Billerica, MA, USA). Tris and β-mercaptoethanol were obtained from Amresco (Solon, OH, USA). 3-(4,5-dimethylthiazol-. 2-yl)-2,5-diphenyl tetrazolium bromide (MTT), SDS, and bis-acrylamide were from USB (Cleveland, OH, USA). Acrylamide and Hybond nitrocellulose were purchased from GE Healthcare Life Sciences (Piscataway, NJ, USA). All other reagents were of the highest analytical grade.

2.2. Animals

All animal studies were carried out in accordance with the “Principles of Laboratory Animal Care” (NIH publication number 80-23, revised 1996) and approved by the local Ethical Committee for Animal Research. Wistar rats of both genders at postnatal day 14 (PND14) were obtained from our own breeding colony at the Universidade Federal de Santa Catarina (UFSC), Brazil. At this developmental stage (PND14), female and male rats do not display differences in hormonal activity, since sexual maturity is not yet reached [24]. Rats were maintained in an air-conditioned room (22–25°C) on a 12-h light/dark cycle with water and food ad libitum.

2.3. Striatal and Hippocampal Slice Preparation and Treatments

Preparation and treatment of striatal and hippocampal slices were performed as previously described [2527]. Briefly, a total of 32 animals were euthanized by decapitation; their encephala were extracted and the striata and hippocampi were immediately dissected (4°C) in HEPES-saline buffer (124 mM NaCl, 4 mM KCl, 1.2 mM MgSO4, 12 mM D-glucose, 1 mM CaCl2, and 25 mM HEPES; pH 7.4), which was previously oxygenated for 30 min. Slices of 400 μm thickness were prepared using a McIlwain Tissue Chopper. In order to obtain a sufficient number of slices, two immature rats (PND14) were used for each of the experiments. The hippocampal slices obtained were pooled and subsequently three slices for each treatment were carefully separated with a brush. The slices were individually preincubated with HEPES-saline buffer (300 μL/slice) for 30 min at room temperature (RT). For the treatments, the HEPES-saline buffer was replaced by fresh buffer in the absence (control) or presence of MnCl2 (1–1,000 μM) and incubated for 3 h at 37°C. These concentrations were chosen based on previous reports, which have used similar concentrations in vitro [22]. The concentrations chosen encompass the physiological (10 μM), threshold of toxicity (100 μM), and toxic (1,000 μM) spectrum based on reports by Suzuki et al. [28] performed in monkeys.

The extended incubations (6 h) required different buffers similar to the conditions used for maintenance of organotypic slice cultures. The maintenance of cell viability under this experimental condition has been previously described [27]. Dissection (4°C) and preincubation (30 min, RT) were performed in Krebs-Ringer bicarbonate buffer (KRB) (122 mM NaCl, 3 mM KCl, 1.2 mM MgSO4, 1.3 mM CaCl2, 0.4 mM KH2PO4, 25 mM NaHCO3, and 10 mM D-glucose). The buffer was bubbled with 95% O2–5% CO2 to pH 7.4. For the treatments, the medium was replaced by a nutritive incubation medium composed of 50% KRB, 50% Dulbecco’s modified Eagle’s medium (DMEM), 20 mM of HEPES, and 100 μg/mL of gentamicin, at 37°C in a 95% O2/5% CO2 atmosphere, in the absence (control) or presence of MnCl2 (1–1,000 μM), and the slices were incubated for 6 h [26, 27].

2.4. Cell Viability

Slice viability was analyzed by the colorimetric MTT [3′-(4,5-dimethylthiazol-2yl) 2,5-diphenyltetrazolium bromide] reduction assay [29]. At the end of the treatments, the medium was removed and the slices (in triplicates) were incubated with 0.5 mg/mL MTT (200 μL) in HEPES-saline buffer (in the case of 3 h treatments) or KRB (6 h treatments). The slices were incubated for 20 minutes at 37°C. Mitochondrial dehydrogenases in viable cells reduce MTT to formazan crystals, which are dissolved in dimethylsulfoxide (DMSO). The absorbance was quantified spectrophotometrically using a microplate reader (  nm). Results are expressed as a percentage of the control (absence of MnCl2).

2.5. Western Blotting Analysis

To access MAPK activation, western blot analysis of slices samples was performed as previously described [25, 30, 31]. Briefly, the slices were solubilized with SDS-stopping solution (4% SDS, 2 mM EDTA, 50 mM Tris, 5% β-mercaptoethanol, pH 6.8) for 5 minutes at 100°C. Aliquots for protein concentration determination were collected before β-mercaptoethanol addition and protein concentration was later determined by the Peterson method [32]. Next, 25 : 100 (v/v) of sample dilution was added (40% glicerol, 25 mM Tris, bromophenol blue, and pH 6.8). Sixty μg of total protein/track were separated by sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) using 10% gels (miniVE Vertical Electrophoresis System, GE Healthcare Life Sciences, Piscataway, NJ, USA), followed by transfer to nitrocellulose membranes using a semidry blotting apparatus (TE 70 SemiPhor Unit, GE Healthcare Life Sciences, Piscataway, NJ, USA) (1.2 mA/cm2; 1 h 30 min) as described by Bjerrum and Heegaard (1988). After blocking with 5% skim milk in Tris buffered saline (TBS) (Tris 10 mM, NaCl 150 mM, pH 7.5) for 1 hour, membranes were incubated overnight (4°C) with primary antibodies to detect the phosphorylated forms of ERK1/2, JNK1/2/3, , and TH, in the dilutions recommended by the manufacturer. Subsequently, membranes were incubated for 1 h at RT with anti-Rabbit IgG HRP conjugate secondary antibodies. All steps were followed by three 5 minutes washing with TBS-T (TBS with the addition of Tween-20 0.1% and pH 7.5). The blots were developed by chemiluminescent reaction. Subsequently, membranes were stripped of the antibodies using a solution of NaOH 0.2 N and then reprobed to detect the total forms (phosphorylated plus nonphosphorylated form) of the target proteins. The bands were quantified using the Scion Image software (Frederick, MD, USA). The ratio of the optic density (OD) of the phosphorylated protein band over the OD of the total protein band was calculated and the phosphorylation level of each protein was determined as a percentage of the control (considered 100%).

The antibody against ERK1/2 detected two bands, one at approximately 44 kDa and the second at approximately 42 kDa, corresponding, respectively, to the two ERK isoforms, ERK1 and ERK2. Anti- detected a single band of approximately 38 kDa; anti-JNK 1/2/3 detected two bands, one at approximately 54 kDa and the second at approximately 46 kDa, corresponding, respectively, to the three JNK isoforms, JNK2/3 and JNK1.

2.6. Statistical Analyses

Statistical analyses were performed by one-way analysis of variance (ANOVA) followed by Duncan’s post hoc test when appropriate using STATISTICA 5.1 software (SS Inc., Tulsa, OK, USA). Differences were considered to be significant when . The values were expressed as mean ± S.E.M.

3. Results

3.1. Assessment of Cell Viability in Striatal and Hippocampal Slices Exposed to Mn

Previous studies show selective neurotoxicity of Mn toward basal ganglia structures, such as the striatum (caudate, putamen, and nucleus accumbens), globus pallidus, and substantia nigra [1]. In this study, in vitro Mn exposure (10–1,000 μM) for 3 or 6 hours did not significantly affect cell viability in either striatal (Figure 1(a)) or hippocampal slices (Figure 1(b)) assessed by MTT. The results for 3 and 6 hours incubations were obtained separately and are expressed as percentage relative to the control.

3.2. MAPKs Modulation in Striatal Slices Exposed to Mn

The phosphorylation levels of ERK1/2, JNK1/2/3, and were assessed in striatal or hippocampal slices isolated from immature rats (PND14) in response to in vitro Mn exposure. Slices were exposed for 3 or 6 h to Mn at concentrations ranging from 10–1,000 μM and then analyzed by western blotting.

Figures 2(a) and 2(b) show that Mn exposure (10 μM, 3 h) significantly increased ERK1 and ERK2 phosphorylation ( %) ( , ) and % ( , ), respectively, in striatal slices. JNK1/2/3 (Figures 2(c) and 2(d)), and (Figures 2(e) and 2(f)) phosphorylation were not significantly different from controls after 3 h exposure to Mn.

When striatal slices were exposed to 1,000 μM Mn for 6 h, significant increases in ERK1 ( %) ( , ), ERK2 ( %) ( , ) (Figures 3(a) and 3(b)), JNK1 ( %) ( , ), and JNK2/3 ( %) ( , ) (Figure 3(d)) phosphorylation were observed. However, only JNK1 ( %) (    ) and JNK2/3 ( %) ( , ) phosphorylation (Figures 3(c) and 3(d)) were significantly increased after exposures to 100 μM Mn and no significant changes were observed in phosphorylation under the same experimental conditions (Figures 3(e) and 3(f)).

3.3. MAPKs Modulation in Hippocampal Slices Exposed to Mn

Hippocampal slices exposed to Mn for 3 h showed a significant increase of ERK1 ( %) ( , ) and ERK2 phosphorylation ( %) ( , ) at 100 μM Mn (Figures 4(a) and 4(b)). Moreover, ERK2 phosphorylation was also significantly increased ( %) ( , ) at the highest Mn concentration tested (1,000 μM). JNK1/2/3 (Figures 4(c) and 4(d)) and (Figures 4(e) and 4(f)) phosphorylation were not modified in the hippocampal slices after 3 h exposure to Mn.

When hippocampal slices were exposed to Mn for 6 h, a significant increase in the phosphorylation of ERK1 ( %) ( , ) and ERK2 ( %) ( , ) (Figures 5(a) and 5(b)), JNK1 ( %) ( , ), and JNK2/3 ( %) ( , ) (Figures 5(c) and 5(d)) were observed at the highest Mn concentration (1,000 μM). No significant changes were observed in phosphorylation under the same experimental conditions (Figures 5(e) and 5(f)).

3.4. Phosphorylation of TH at Ser40 in Striatal Slices Exposed to Mn

TH is the rate-limiting enzyme for dopamine (DA) synthesis. Medium- and long-term modulation of TH activity occurs by regulation of gene expression and in the short-term by regulation of enzyme activity. Phosphorylation on serine residues, by several enzymes, is the primary mechanism of short-term TH activity regulation [33, 34]. Previous studies in PC12 cells demonstrated increased Ser40 phosphorylation and activation of TH in response to Mn [23]. However, in our experimental protocol (with tissue slices) no significant changes in TH-Ser40 phosphorylation in response to Mn (10–1,000 μM) exposure were observed (Figure 6).

4. Discussion

Recent data from our group demonstrated that developmental Mn exposure from postnatal days 8–12 (PND8–12) altered the activity of key cell signaling elements, causing increased phosphorylation of DARPP-32-Thr-34, ERK1/2, and AKT in the striatum of rats on PND14 [12]. Additionally, in the same experimental protocol, Mn impaired motor coordination later at the 3rd, 4th, and 5th week of life. These results were in line with recent evidence indicating that MAPK pathways might be involved in the neurotoxicity induced by Mn in various experimental models, such as mesencephalic cells [16], PC12 cells [15, 23, 35], microglial cells [36, 37], primary astrocyte culture [17], and in vivo developmental exposure [12, 13]. However, the current knowledge on Mn-induced neurotoxicity does not allow for stating whether changes in MAPK signaling pathways represent cause or consequence of Mn-induced cell toxicity. In an attempt to investigate if Mn can modulate MAPK signaling pathways in conditions where cells are still completely viable, we took advantage of a slice-based model to evaluate Mn-induced effects in vitro with particular emphasis on striatal and hippocampal tissues. Employing experimental conditions (Mn concentration and exposure time) that do not cause significant cell death (evaluated by the MTT assay; Figure 1), we observed that both striatal and hippocampal slices showed significant changes in MAPKs phosphorylation.

Our results showed that slice incubation with MnCl2 did not induce significant changes in cell viability (Figure 1). This finding corroborates findings by Sistrunk et al. [22], who failed to observe Mn-induced cell death in an in vitro model of rat striatal slices exposed to MnCl2 (10–1,000 μM) for 4 hours. However, a decrease in cell viability in vitro was demonstrated in DAergic PC12 cells [14, 23] after exposure to high Mn concentrations for extended periods (24–48 h). It needs to be taken into account that the cell viability in the present work was assessed only by the MTT test. Other methods such as lactate dehydrogenase (LDH) or neutral red could be tested in future works. Nevertheless, as mentioned above, it needs to be considered that studies in pure PC12 cultures are void of glial cells, which are known modulators of Mn CNS homeostasis. Astrocytes accumulate higher levels of Mn than neurons and may be an initial site for Mn-induced damage, thus, lowering the neuronal burden of Mn [8]. Furthermore, the slice model provides only a short time window for metal exposure (in our case a maximum of 6 hours) beyond which the cell viability is compromised [27]. Lead (Pb), another metal widely recognized as a neurotoxicant [38], has also been evaluated in the slices model [25]. No changes in cell viability were observed after the treatment of hippocampal slices from PND14 rats with Pb acetate. However, phosphorylation levels of ERK and were increased. These results indicate that even though cell viability is not compromised, toxic metals may still cause changes in cells signaling pathways in vitro that may disturb cellular function [25].

Our results showed an increase in ERK phosphorylation in striatal slices exposed to a low Mn concentration (10 μM) for 3 hours (Figure 2(b)). ERK and JNK phosphorylation also increased in striatal slices exposed to 100 and 1,000 μM Mn for 6 hours (Figures 3(b) and 3(d), resp.). Of note, these changes in MAPK signaling pathways were observed in slices completely viable (no changes in the MTT assay), indicating that altered intracellular MAPKs signaling pathways may represent an early event of Mn action in the slices. ERK1/2 activation has also been observed in the striatum of immature rats (PND14) developmentally exposed to Mn (PND8–12) [12]. Therefore, it appears that activation of ERK1/2 by Mn may be an early and conserved mechanism observed both in vitro and in vivo.

The majority of in vitro studies concerning the effects of Mn on cell signaling pathways were conducted in cell culture models [23, 39]. However, neuroglial interactions may play important roles in the modulation of neurotoxic processes, including those triggered by metals [40, 41]. Thus, in vitro studies, which in general are focused on single cell type (e.g., neuron or astrocyte alone), fail to take into account toxic events that are dependent upon neuronal and glial interactions. In contrast, tissue slices from rat brain maintain the natural extracellular matrix, neuronal connectivity, and neuroglial interactions, providing an appropriate experimental model for studies on acute neurotoxic events [42, 43]. The model of 400 μm thick brain slices is well established [42, 44] and has been used for in vitro studies on the neurotoxicity of metals, such as cadmium (Cd) [30] and Pb [25].

Striatal slices are rich in DAergic neurons, in contrast to hippocampal slices. Of particular importance, Mn shows selective neurotoxicity to DAergic neurons by mechanisms that have yet to be fully defined but possibly involve interaction with DA, leading to its oxidation forming toxic quinones and consequent oxidative stress [4547]. A recent study in Caenorhabditis elegans showed that extracellular and not intracellular DA is responsible for Mn-induced DAergic neurodegeneration [48]. Moreover, it is known that the striatum expresses higher levels of DMT-1, which is the predominant transporter for divalent Mn into cells [49]. Therefore, the presence of DAergic neurons and DMT1 in striatal slices may explain, at least in part, the significant modulation of MAPKs by a relative low Mn concentration in striatal tissue as compared to hippocampus.

With respect to the susceptibility of hippocampal slices to Mn, we noted increased ERK1/2 phosphorylation following exposure of hippocampal slices to 100 and 1,000 μM Mn for 3 hours (Figure 4(b)). ERK and JNK also showed increased phosphorylation in hippocampal slices exposed to 1,000 μM Mn for 6 h (Figures 5(b) and 5(d), resp.). In a recent study, the hippocampus was studied as a site for Mn neurotoxicity in vivo, since Mn exposure increased the levels of thiobarbituric acid reactive species (TBARS), diminished total thiol content, and increased superoxide dismutase and catalase activity, indicating oxidative stress within this structure [50]. Therefore, although the basal ganglia are the most susceptible sites to Mn neurotoxicity, it is also evident that Mn may cause broad spectrum neuropathological changes in both neurons and glia in other brain regions, which may account for some of the nonmotor symptoms associated with this disorder [1].

Given the (1) importance of TH in controlling DA levels in neurons, (2) the involvement of DA metabolism in Mn neurotoxicity, as well as (3) a plethora of studies showing TH activity modulation and Ser40 phosphorylation by Mn [23, 39], we investigated Mn’s effects on TH Ser40 phosphorylation in striatal slices from immature rats. This site is phosphorylated by protein kinase A (PKA) and protein kinase C (PKC), increasing TH activity. Ser40 dephosphorylation by protein phosphatase 2A (PP2A) results in decreased TH activity [33]. Our results showed no significant alteration in TH phosphorylation at Ser40 (Figure 6). This result indicates that in immature striatal slices Mn does not act in an analogous way to PC12 cells exposed to Mn (100 μM). In the latter study, a sustained TH-Ser40 phosphorylation (6–24 h) was observed, independent from H2O2 production and in the absence of significant changes in cell viability [23].

Thus, based on our and previous studies, it can be inferred that Mn requires longer exposure periods to induce cell death in slices. However, important molecular changes were observed within short periods after Mn exposure, such as the activation of ERK1/2 and JNK1/2/3 signaling pathway (Figures 25). These findings are in agreement with those previously reported by our group in a model of developmentally exposed rats where ERK1/2 activation but not JNK1/2/3 was noted [12]. Thus, striatal slices of immature rats exposed in vitro to Mn reproduce (at least in part) the changes observed in vivo.

5. Conclusions

A key finding in this study is the Mn-dependent activation of ERK1/2 and JNK1/2/3 in striatal and hippocampal slices with no significant changes in cell viability. This finding indicates that MAPKs activation may represent an important primary event that precedes the deleterious effects of Mn on the cellular viability. Extrapolating our data to in vivo conditions, one would posit that Mn is able to modulate the activation of MAPKs in tissues that maintain their metabolic competence and viability. The physiological significance of such activation represents a research topic that needs further attention.

Conflict of Interests

None of the authors has a known or perceived conflict of interests with the contents of this paper.


This work was supported by the Conselho Nacional de Desenvolvimento Científico e Tecnológico (CNPq) Brazil (no. 305194/2010-0); the Coordenação de Aperfeiçoamento de Pessoal de Nível Superior (CAPES)/PROCAD; the National Institute of Science and Technology (INCT) for Excitotoxicity and Neuroprotection; the Fundação de Amparo a Pesquisa de Santa Catarina (FAPESC); FAPESC/PRONEX—Núcleo de Excelência em Neurociências Aplicadas de Santa Catarina (NENASC); and IBN.Net/CNPq. Marcelo Farina, Roger Walz, and Rodrigo Bainy Leal are recipient of Research Scholarship from CNPq. Michael Aschner was supported in part by Grants from the National Institutes of Health ES R01 10563 and ES P30 00267. The funding agencies had no role in study design, data collection and analysis, decision to publish, or preparation of the paper.


  1. M. Aschner, K. M. Erikson, E. H. Hernández, and R. Tjalkens, “Manganese and its role in Parkinson's disease: from transport to neuropathology,” NeuroMolecular Medicine, vol. 11, no. 4, pp. 252–266, 2009. View at: Publisher Site | Google Scholar
  2. T. R. Guilarte, “Manganese and Parkinson's disease: a critical review and new findings,” Environmental Health Perspectives, vol. 118, no. 8, pp. 1071–1080, 2010. View at: Publisher Site | Google Scholar
  3. T. E. Gunter, C. E. Gavin, M. Aschner, and K. K. Gunter, “Speciation of manganese in cells and mitochondria: a search for the proximal cause of manganese neurotoxicity,” NeuroToxicology, vol. 27, no. 5, pp. 765–776, 2006. View at: Publisher Site | Google Scholar
  4. T. R. Guilarte, N. C. Burton, T. Verina et al., “Increased APLP1 expression and neurodegeneration in the frontal cortex of manganese-exposed non-human primates,” Journal of Neurochemistry, vol. 105, no. 5, pp. 1948–1959, 2008. View at: Publisher Site | Google Scholar
  5. R. M. Molina, S. Phattanarudee, J. Kim et al., “Ingestion of Mn and Pb by rats during and after pregnancy alters iron metabolism and behavior in offspring,” NeuroToxicology, vol. 32, no. 4, pp. 413–422, 2011. View at: Publisher Site | Google Scholar
  6. C. H. Kern and D. R. Smith, “Preweaning Mn exposure leads to prolonged astrocyte activation and lasting effects on the dopaminergic system in adult male rats,” Synapse, vol. 65, no. 6, pp. 532–544, 2011. View at: Publisher Site | Google Scholar
  7. J. A. Moreno, E. C. Yeomans, K. M. Streifel, B. L. Brattin, R. J. Taylor, and R. B. Tjalkens, “Age-dependent susceptibility to manganese-induced neurological dysfunction,” Toxicological Sciences, vol. 112, no. 2, pp. 394–404, 2009. View at: Publisher Site | Google Scholar
  8. L. E. Gonzalez, A. A. Juknat, A. J. Venosa, N. Verrengia, and M. L. Kotler, “Manganese activates the mitochondrial apoptotic pathway in rat astrocytes by modulating the expression of proteins of the Bcl-2 family,” Neurochemistry International, vol. 53, no. 6–8, pp. 408–415, 2008. View at: Publisher Site | Google Scholar
  9. Y. Liu, D. S. Barber, P. Zhang, and B. Liu, “Complex II of the mitochondrial respiratory chain is the key mediator of divalent manganese-induced hydrogen peroxide production in microglia,” Toxicological Sciences, vol. 132, no. 2, pp. 298–306, 2013. View at: Publisher Site | Google Scholar
  10. H. Yoon, D.-S. Kim, G.-H. Lee, K.-W. Kim, H.-R. Kim, and H.-J. Chae, “Apoptosis induced by manganese on neuronal SK-N-MC cell line: Endoplasmic Reticulum (ER) stress and mitochondria dysfunction,” Environmental Health and Toxicology, vol. 26, Article ID e2011017, 2011. View at: Publisher Site | Google Scholar
  11. D. Milatovic, S. Zaja-Milatovic, R. C. Gupta, Y. Yu, and M. Aschner, “Oxidative damage and neurodegeneration in manganese-induced neurotoxicity,” Toxicology and Applied Pharmacology, vol. 240, no. 2, pp. 219–225, 2009. View at: Publisher Site | Google Scholar
  12. F. M. Cordova, A. S. Aguiar Jr., T. V. Peres et al., “In vivo manganese exposure modulates Erk, Akt and Darpp-32 in the striatum of developing rats, and impairs their motor function,” PLoS ONE, vol. 7, no. 3, Article ID e33057, 2012. View at: Publisher Site | Google Scholar
  13. F. M. Cordova, A. S. Aguiar Jr., T. V. Peres et al., “Manganese-exposed developing rats display motor deficits and striatal oxidative stress that are reversed by Trolox,” vol. 87, no. 7, pp. 1231–1244, 2013. View at: Publisher Site | Google Scholar
  14. Y. Hirata, T. Meguro, and K. Kiuchi, “Differential effect of nerve growth factor on dopaminergic neurotoxin-induced apoptosis,” Journal of Neurochemistry, vol. 99, no. 2, pp. 416–425, 2006. View at: Publisher Site | Google Scholar
  15. Y. Ito, K. Oh-hashi, K. Kiuchi, and Y. Hirata, “p44/42 MAP kinase and c-Jun N-terminal kinase contribute to the up-regulation of caspase-3 in manganese-induced apoptosis in PC12 cells,” Brain Research, vol. 1099, no. 1, pp. 1–7, 2006. View at: Publisher Site | Google Scholar
  16. K. Prabhakaran, G. D. Chapman, and P. G. Gunasekar, “α-synuclein overexpression enhances manganese-induced neurotoxicity through the NF-κB-mediated pathway,” Toxicology Mechanisms and Methods, vol. 21, no. 6, pp. 435–443, 2011. View at: Publisher Site | Google Scholar
  17. Z. Yin, J. L. Aschner, A. P. dos Santos, and M. Aschner, “Mitochondrial-dependent manganese neurotoxicity in rat primary astrocyte cultures,” Brain Research, vol. 1203, pp. 1–11, 2008. View at: Publisher Site | Google Scholar
  18. E. K. Kim and E.-J. Choi, “Pathological roles of MAPK signaling pathways in human diseases,” Biochimica et Biophysica Acta, vol. 1802, no. 4, pp. 396–405, 2010. View at: Publisher Site | Google Scholar
  19. G. M. Thomas and R. L. Huganir, “MAPK cascade signalling and synaptic plasticity,” Nature Reviews Neuroscience, vol. 5, no. 3, pp. 173–183, 2004. View at: Google Scholar
  20. T. R. Guilarte, N. C. Burton, J. L. McGlothan et al., “Impairment of nigrostriatal dopamine neurotransmission by manganese is mediated by pre-synaptic mechanism(s): implications to manganese-induced parkinsonism,” Journal of Neurochemistry, vol. 107, no. 5, pp. 1236–1247, 2008. View at: Publisher Site | Google Scholar
  21. K. M. Erikson, K. Thompson, J. Aschner, and M. Aschner, “Manganese neurotoxicity: a focus on the neonate,” Pharmacology & Therapeutics, vol. 113, no. 2, pp. 369–377, 2007. View at: Publisher Site | Google Scholar
  22. S. C. Sistrunk, M. K. Ross, and N. M. Filipov, “Direct effects of manganese compounds on dopamine and its metabolite Dopac: an in vitro study,” Environmental Toxicology and Pharmacology, vol. 23, no. 3, pp. 286–296, 2007. View at: Publisher Site | Google Scholar
  23. T. Posser, J. L. Franco, L. Bobrovskaya, R. B. Leal, P. W. Dickson, and P. R. Dunkley, “Manganese induces sustained Ser40 phosphorylation and activation of tyrosine hydroxylase in PC12 cells,” Journal of Neurochemistry, vol. 110, no. 3, pp. 848–856, 2009. View at: Publisher Site | Google Scholar
  24. P. Sengupta, “The laboratory rat: relating its age with human's,” International Journal of Preventive Medicine, vol. 4, no. 6, pp. 624–630, 2013. View at: Google Scholar
  25. F. M. Cordova, A. L. S. Rodrigues, M. B. O. Giacomelli et al., “Lead stimulates ERK1/2 and p38MAPK phosphorylation in the hippocampus of immature rats,” Brain Research, vol. 998, no. 1, pp. 65–72, 2004. View at: Publisher Site | Google Scholar
  26. A. V. Jacques, D. K. Rieger, M. Maestri et al., “Lectin from Canavalia brasiliensis (ConBr) protects hippocampal slices against glutamate neurotoxicity in a manner dependent of PI3K/Akt pathway,” Neurochemistry International, vol. 62, no. 6, pp. 836–842, 2013. View at: Publisher Site | Google Scholar
  27. S. Molz, H. Decker, T. Dal-Cim et al., “Glutamate-induced toxicity in hippocampal slices involves apoptotic features and p38MAPK signaling,” Neurochemical Research, vol. 33, no. 1, pp. 27–36, 2008. View at: Publisher Site | Google Scholar
  28. Y. Suzuki, T. Mouri, and Y. Suzuki, “Study of subacute toxicity of manganese dioxide in monkeys,” Tokushima Journal of Experimental Medicine, vol. 22, pp. 5–10, 1975. View at: Google Scholar
  29. Y. Liu, D. A. Peterson, H. Kimura, and D. Schubert, “Mechanism of cellular 3-(4,5-dimethylthiazol-2-yl)-2,5- diphenyltetrazolium bromide (MTT) reduction,” Journal of Neurochemistry, vol. 69, no. 2, pp. 581–593, 1997. View at: Google Scholar
  30. A. P. Rigon, F. M. Cordova, C. S. Oliveira et al., “Neurotoxicity of cadmium on immature hippocampus and a neuroprotective role for p38MAPK,” NeuroToxicology, vol. 29, no. 4, pp. 727–734, 2008. View at: Publisher Site | Google Scholar
  31. R. B. Leal, F. M. Cordova, L. Herd, L. Bobrovskaya, and P. R. Dunkley, “Lead-stimulated p38MAPK-dependent Hsp27 phosphorylation,” Toxicology and Applied Pharmacology, vol. 178, no. 1, pp. 44–51, 2002. View at: Publisher Site | Google Scholar
  32. G. L. Peterson, “A simplification of the protein assay method of Lowry et al. Which is more generally applicable,” Analytical Biochemistry, vol. 83, no. 2, pp. 346–356, 1977. View at: Google Scholar
  33. P. R. Dunkley, L. Bobrovskaya, M. E. Graham, E. I. Von Nagy-Felsobuki, and P. W. Dickson, “Tyrosine hydroxylase phosphorylation: regulation and consequences,” Journal of Neurochemistry, vol. 91, no. 5, pp. 1025–1043, 2004. View at: Publisher Site | Google Scholar
  34. S. C. Kumer and K. E. Vrana, “Intricate regulation of tyrosine hydroxylase activity and gene expression,” Journal of Neurochemistry, vol. 67, no. 2, pp. 443–462, 1996. View at: Google Scholar
  35. T. Cai, H. Che, T. Yao et al., “Manganese induces Tau hyperphosphorylation through the activation of ERK MAPK pathway in PC12 cells,” Toxicological Sciences, vol. 119, no. 1, pp. 169–177, 2011. View at: Publisher Site | Google Scholar
  36. J.-H. Bae, B.-C. Jang, S.-I. Suh et al., “Manganese induces inducible nitric oxide synthase (iNOS) expression via activation of both MAP kinase and PI3K/Akt pathways in BV2 microglial cells,” Neuroscience Letters, vol. 398, no. 1-2, pp. 151–154, 2006. View at: Publisher Site | Google Scholar
  37. P. L. Crittenden and N. M. Filipov, “Manganese modulation of MAPK pathways: effects on upstream mitogen activated protein kinase kinases and mitogen activated kinase phosphatase-1 in microglial cells,” Journal of Applied Toxicology, vol. 31, no. 1, pp. 1–10, 2011. View at: Publisher Site | Google Scholar
  38. P. Grandjean and P. Landrigan, “Developmental neurotoxicity of industrial chemicals,” The Lancet, vol. 368, no. 9553, pp. 2167–2178, 2006. View at: Publisher Site | Google Scholar
  39. D. Zhang, A. Kanthasamy, V. Anantharam, and A. Kanthasamy, “Effects of manganese on Tyrosine Hydroxylase (TH) activity and TH-phosphorylation in a dopaminergic neural cell line,” Toxicology and Applied Pharmacology, vol. 254, no. 2, pp. 65–71, 2011. View at: Publisher Site | Google Scholar
  40. N. M. Filipov and C. A. Dodd, “Role of glial cells in manganese neurotoxicity,” Journal of Applied Toxicology, vol. 32, no. 5, pp. 310–317, 2012. View at: Publisher Site | Google Scholar
  41. F. Zhao, T. Cai, M. Liu, G. Zheng, W. Luo, and J. Chen, “Manganese induces dopaminergic neurodegeneration via microglial activation in a rat model of manganism,” Toxicological Sciences, vol. 107, no. 1, pp. 156–164, 2009. View at: Publisher Site | Google Scholar
  42. C.-X. Gong, T. Lidsky, J. Wegiel, I. Grundke-Iqbal, and K. Iqbal, “Metabolically active rat brain slices as a model to study the regulation of protein phosphorylation in mammalian brain,” Brain Research Protocols, vol. 6, no. 3, pp. 134–140, 2001. View at: Publisher Site | Google Scholar
  43. Y. Hirata and T. Nagatsu, “Rotenone and CCCP inhibit tyrosine hydroxylation in rat striatal tissue slices,” Toxicology, vol. 216, no. 1, pp. 9–14, 2005. View at: Publisher Site | Google Scholar
  44. R. Rodnight and R. Leal, “Regional variations in protein phosphorylating activity in rat brain studied in micro-slices labeled with [32P]phosphate,” Journal of Molecular Neuroscience, vol. 2, no. 2, pp. 115–122, 1990. View at: Publisher Site | Google Scholar
  45. G. Díaz-Véliz, S. Mora, P. Gómez et al., “Behavioral effects of manganese injected in the rat substantia nigra are potentiated by dicumarol, a DT-diaphorase inhibitor,” Pharmacology Biochemistry and Behavior, vol. 77, no. 2, pp. 245–251, 2004. View at: Publisher Site | Google Scholar
  46. E. J. Martinez-Finley, C. E. Gavin, M. Aschner, and T. E. Gunter, “Manganese neurotoxicity and the role of reactive oxygen species,” Free Radical Biology and Medicine, vol. 62, pp. 65–75, 2013. View at: Publisher Site | Google Scholar
  47. K. Prabhakaran, D. Ghosh, G. D. Chapman, and P. G. Gunasekar, “Molecular mechanism of manganese exposure-induced dopaminergic toxicity,” Brain Research Bulletin, vol. 76, no. 4, pp. 361–367, 2008. View at: Publisher Site | Google Scholar
  48. A. Benedetto, C. Au, D. S. Avila, D. Milatovic, and M. Aschner, “Extracellular dopamine potentiates Mn-induced oxidative stress, lifespan reduction, and dopaminergic neurodegeneration in a BLI-3-dependent manner in caenorhabditis elegans,” PLoS Genetics, vol. 6, no. 8, Article ID e1001084, 2010. View at: Publisher Site | Google Scholar
  49. C. Au, A. Benedetto, and M. Aschner, “Manganese transport in eukaryotes: the role of DMT1,” NeuroToxicology, vol. 29, no. 4, pp. 569–576, 2008. View at: Publisher Site | Google Scholar
  50. E. N. Martins, N. T. C. Pessano, L. Leal et al., “Protective effect of Melissa officinalis aqueous extract against Mn-induced oxidative stress in chronically exposed mice,” Brain Research Bulletin, vol. 87, no. 1, pp. 74–79, 2012. View at: Publisher Site | Google Scholar

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