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Int. J. Mol. Sci. 2014, 15(2), 2475-2493; doi:10.3390/ijms15022475
Abstract: In the present work, we have studied whether cell death could be induced in cortical neurons from rats subjected to different period of O2 deprivation and low glucose (ODLG). This “in vitro” model is designed to emulate the penumbra area under ischemia. In these conditions, cortical neurons displayed loss of mitochondrial respiratory ability however, nor necrosis neither apoptosis occurred despite ROS production. The absence of cellular death could be a consequence of increased antioxidant responses such as superoxide dismutase-1 (SOD1) and GPX3. In addition, the levels of reduced glutathione were augmented and HIF-1/3α overexpressed. After long periods of ODLG (12–24 h) cortical neurons showed cellular and mitochondrial membrane alterations and did not recuperate cellular viability during reperfusion. This could mean that therapies directed toward prevention of cellular and mitochondrial membrane imbalance or cell death through mechanisms other than necrosis or apoptosis, like authophagy, may be a way to prevent ODLG damage.
The brain requires a continuous supply of oxygen and glucose to maintain central nervous system (CNS) functions. The deprivation resulting from stroke or respiratory failure, can rapidly lead to transient or permanent neuronal injury as consequence of reduced energy bioavailability; pump function or membrane integrity . Cerebral ischemia is an important cause of death and working disability in humans [2,3]. Caspase-3, an effecter enzyme involved in apoptosis , may contribute to the pathophysiology of cerebral ischemia. Other mechanisms including inflammation and angiogenesis together with ROS formation contribute to cell death in stroke [5–8]. However, ROS production protects against H2O2 toxicity  and may regulate signal transduction pathways under physiological [10,11] and pathological conditions [12–15]. However, controversial data suggests that glutamate may play a neurotoxic role in cerebral ischemia [16–23].
Cerebral artery occlusion can induce apoptosis or necrotic cell death. This occlusion may induce differential damages depending of the lack of O2 and nutrients. These zones are the “core” area and the “penumbra” area, which are rendered functionally silent but retain alive cells . Many studies have shown that neurons from the ischemic penumbra undergo apoptosis rather than necrosis, suggesting that this area can be potentially and functionality recovered [25–27], however, the molecular mechanisms involved are not well known.
Hypoxia-inducible factors (HIFs) are transcriptional mediators of adaptive responses that decrease oxygen availability, a characteristic of ischemic-hypoxia conditions . HIFs are ubiquitously expressed in several mammalian cell types . Since its discovery, the HIFs cascade has been extensively studied and plays a role in both physiological, as tissue repair, and pathological process [30–32], as ischemia [33,34].
The model of oxygen deprivation-low glucose (ODLG) chosen for our study is a reliable and validated method to study cellular damage in cortical neurons subjected to partial ischemia (penumbra area). In our study, cultured cortical neurons were subjected to oxygen-deprivation and low glucose (ODLG model). We studied whether neuronal damage, at different ODLG times (1, 3, 5, 12, and 24 h) could exist under these vulnerability conditions, by evaluating whether (1) ROS formation and expression of antioxidant enzymes (SOD-1 and GPX3) together with the mitochondrial enzyme cytochrome oxidase (CO) might be differentially regulated under ODLG; (2) to study whether HIF-1/3α stabilization could prevent neuronal loss in these cortical neurons; (3) evaluate whether cellular and membrane mitochondrial integrity were affected by measuring membrane potential after ODLG as well as (4) possible cellular dysfunctions of neurotransmission during reperfusion by testing Asp, Glu, Gly and GABA release by HPLC.
2.1. Presence of “HIF” Factor during Hypoxia
The first objective was to demonstrate whether the cortical neurons cultured, under hypoxia, are truly under anoxic conditions. It has been reported that transcription factors (HIF) can be induced in cellular and animal models of cerebral ischemia [35,36]; consequently, the presence of this factor in our preparations was checked by RT-PCR. Data in Figure 1 indicate that under our experimental conditions, cortical neurons significantly upregulated HIF-1α and HIF-3α transcription factors. Reperfusion reversed HIF-1α and HIF-3α upregulation although the values were always higher than the controls.
2.2. ROS Formation
Since oxygen radicals (ROS) are suspected to be involved in cellular injury and death, we analyzed whether hypoxia and hypoglycemia (ODLG) could modulate ROS production “in vitro”. Results in Figure 2 indicate that cortical neurons subjected to these hypoxic and hypoglycemic conditions, generated ROS at the moment in which the cells were in a normal atmosphere. This ROS production increased progressively under hypoxia. In addition, when these neurons were subjected to 24 h of reperfusion, ROS production was completely reversed, reaching values similar to those in control cells.
2.3. Cell Viability
Since ROS formation could play a pivotal role in cell death, cell viability was tested by two methods, crystal violet, which measures cell viability (Figure 3A) and the XTT assay, which measures the metabolic activity of these neurons (Figure 3B). The crystal violet test showed an absence of neuronal loss in cortical neurons at all studied times (Figure 3A). However, the XTT assay showed a time-dependent loss of cell viability (Figure 3B). Reperfusion did not reverse the loss of viability in cells subjected to 5 to 24 h of ODLG, although at shorter times showed levels similar to controls.
2.4. Cellular Death (LDH Assay)
The lack of cellular viability in the XTT assay has two interpretations: (1) cell death or (2) loss of metabolic ability. In order to check these options, LDH activity was also measured to evaluate necrotic death and caspase-3 activation (a sensor of apoptosis) was quantified. Results in Figure 4A show that cortical neurons at 1 to 24 h of ODLG did not significantly increase their LDH release.
2.5. Caspase-3 Activation
Regarding caspase-3 activity, there was a significant proportional decline in caspase-3 activity with the increase in ODLG times (Figure 4B). Reperfusion did not reverse the caspase-3 inactivation produced by 1–5 h of ODLG. In fact, caspase 3 activity was even lower during reperfusion at this time. The inhibitory effects were more evident after 1–3 h of ischemia. Caspase-3 was significantly overproduced at 24 h during reperfusion as compared to values obtained in the non reperfused cells.
2.6. Cytochrome Oxidase
Results in Figure 5 show that cytochrome oxidase activity (CO), the terminal enzyme of the respiratory chain, decreased during the first hour of ODLG but returned to basal values at longer hypoxia times. During reperfusion, CO decreased at 1 h of ODLG and reached values close to control levels at 3 to 48 h of ODLG.
2.7. Possible Mechanisms which Protect against ROS Damage
As our results do not seem to indicate the existence of cellular death, even despite the high ROS formation, it seems possible that cortical neurons were able to activate defense mechanisms against ROS levels. In fact, glutathione (Figure 6), SOD1 and GPX3 (Figure 7A,B) levels were significantly increased during the first 24 h of ODLG treatment. At 48 h of ODLG, glutathione reached values similar to controls. Reperfusion reversed the SOD1 and GPX3 upregulation although these values still remained higher than in controls (Figure 7A,B). Conversely, during reperfusion, when cells were subjected to 1 to 5 h of hypoxia, glutathione levels were higher than in controls. However, these values were similar to controls at 24 and 48 h of ischemia (Figure 6).
2.8. Cellular and Mitochondrial Membrane Potential
Twenty-four h of hypoxia plus hypoglycemia enhanced cellular membrane potential, suggesting that membrane depolarization was induced by ODLG (Figure 8A). However, low levels of ODLG did not alter the cellular membrane potential. A similar effect was observed in the mitochondrial membrane potential (PMM), which was increased at 12 h of ODLG (Figure 8B), again suggesting depolarization. These effects were not reversed during reperfusion. Shorter ODLG treatment times (1–3 h) did not affect the mitochondrial membrane potential.
2.9. Cellular Functionality (Amino Acid Release)
Finally, since neurotransmission regulates neuronal function, we used HPLC to measure amino acid neurotransmitter release mediated by high KCl in neurons subjected to ODLG for 24 h as well as in controls neurons (Figure 9). Our data indicate that Gly and GABA release were affected as compared to control release in controls. Gly release was higher in control than in ODLG-treated neurons; however the high KCl-induced GABA release was higher in treated neurons as compared to their controls. Nevertheless, ODLG treatment did not affect Asp and Glu release, suggesting that ischemia had only affected inhibitory synapses “in vitro”.
3.1. HIF1α and HIF3α Are Upregulated during ODLG
Our data clearly demonstrate that, under ODLG hypoxia factors HIF1α and HIF3α are upregulated in cortical neurons “in vitro”. This suggests that cortical neurons could develop adaptative responses to O2 deprivation “in vitro”. Although HIF1α levels were lower during reperfusion, they were still higher than in control conditions. In concordance with our findings, several authors have reported that HIF 1α and HIF 3α upregulation can prevent cell death from hypoxia [37,38]. Wu et al.  point out that HIF-1α contributes to early brain injury (EBI) after subarachnoid hemorrhage consisting of cell apoptosis, blood-brain-barrier (BBB) disruption, and brain edema through VEGF upregulation. These detrimental effects were prevented in the presence of the VEGF inhibitor, 2ME2. Our findings suggest that HIF-1α and HIF-3α upregulation may lead to adaptative responses against O2 deprivation in cortical neurons during hypoxia and even during reperfusion because although during this time the levels of HIF-1α and HIF-3α were decreased, the levels of these molecules were slightly higher than in controls.
3.2. ROS Generation and Antioxidant Mechanisms
Unexpectedly, cortical neurons were able to survive in our experimental conditions of ODLG despite the very high ROS production. Thus, we are interested to understand the mechanisms involved in cell protection during this time. Our data indicate that increased glutathione together with SOD1 and GPX3 overproduction under ODLG and even during reperfusion may prevent ROS-mediated damage in cortical neurons “in vitro”. In support of the antioxidant effects observed in our study, Chen et al.  showed that SOD1 was increased during the ischemia in astrocytes culture following oxygen glucose deprivation and reperfusion.
Thus, SOD-1 overexpression may be an essential antioxidant mechanism that prevents neuronal death. Another study in rabbit spinal cords agreed with our findings and indicated that SOD1 protected neuron from spinal ischemic damage by both decreasing lipid peroxidation and maintaining catalase levels .
Collectively, these observations suggest that SOD-1 together with GPX3 overexpression is an adaptative response to oxygen deprivation that also occurred in our study. The reduced antioxidant SOD1 and GPX3 levels observed during reperfusion could decrease antioxidant responses during this time; this would coincide with strong caspase-3 activation during the reperfusion of cortical neurons subjected to ODLG during 24 h in the present study.
Another point deserving mention is the formation of ROS during hypoxia/reperfusion. ROS formation requires O2 and, under O2 deprivation (hypoxia), cortical neurons are in an atmosphere of 95% N2/5% CO2. ROS formation during hypoxia has been reported by several authors, who demonstrated ROS generation in complex III of the mitochondria respiratory chain during hypoxia . In our opinion, the presence of ROS during hypoxia would be possible because during this process, NADH may accumulate. At the moment that cells are rescued from hypoxia, they have enough O2 to produce ROS despite the recent hypoxic conditions. Thus, ROS would not be formed during hypoxia although NADH might further accumulate. In fact, Livnat et al.  found increased NADH levels in the core and penumbra areas.
3.3. Cytochrome Oxidase and ODLG
During ODLG, cytochrome oxidase is lower during the first hour of hypoxia in cortical neurons but afterwards the enzyme shows a progressive recuperation in which it can even reach values similar to the control. This rise could reflect adaptative responses under vulnerability conditions. Cellular adaptation during ischemia has been previously reported by others who showed that preconditioning can protect against subsequent cellular insults [44–46].
3.4. ODLG and Cellular Death
Although neuronal death by necrosis or apoptosis did not occur under ODLG conditions, there were deficits in physiological cellular respiration together with defective neurotransmission that could affect normal neuronal function. The decreases in metabolic ability generated during reperfusion could be due to ATP depletion. If ATP levels were depleted, caspase-3 might not be activated during reperfusion (as occurred in our experiments). As a consequence, neuronal survival could be preserved during this period such as has been reported by Mattson and coworkers . ATP depletion in cortical neurons during oxygen glucose deprivation (OGD) has been reported by others [48,49]. The lack of ATP does not necessarily induce cell death; thus, Yager et al. , studying hypoxic-ischemic damage in astrocytes, found that low ATP was not responsible for cell death. On the other hand, the lethargic state of cortical neurons during ODLG observed in our study by the XTT assay may protect them since such mechanisms can save energy, nutrients and O2 under vulnerable conditions. However, the lack of neuronal viability during reperfusion after 5 and 24 h of ODLG in our study suggests that: (1) there was cellular death or (2) there was an absence of recovery of the normal status during reperfusion. Through the crystal violet test or LDH and caspase-3 assays, our results indicated the absence of cell death by necrosis or apoptosis after 5 to 24 h of ODLG. Thus, we should not exclude the possibility that autophagy could have occurred during this time period. In fact, Arce et al.  showed that cortical neurons subjected to oxygen-glucose-deprivation (OGD) regulated BCL3, a protein involved in autophagy. Moreover, Zhang et al.  have reported that cerebral ischemia-reperfusion induces autophagy as a protective mechanism against neuronal injury.
3.5. ODLG and Cellular Malfunction
Additionally, cortical neurons may malfunction after a long period of ODLG since defective neurotransmission was detected together with dysfunctions in cellular and mitochondrial membrane potentials. Reperfusion after ischemia is a critical period that can lead to cell death as a consequence of mitochondrial membrane alterations during ODLG. In our study, the mitochondrial membrane potential increased at 12 h of ischemia, indicating membrane depolarization. However, this increase remained high after 24 h of reperfusion. These findings suggest that mitochondrial alterations cannot be reversed by reperfusion after a long ODLG treatment, so, the use of membrane protectors could preserve cellular integrity during this period. Our results suggest that mitochondrial alterations after ODLG may contribute to neuronal vulnerability even though apoptosis was not observed in our study. On the other hand, our results also show cellular membrane depolarization after 24 h of ODLG. This could affect neurotransmitter release (mainly glutamate) [47,48] under anoxia and hypoglycemia. Nevertheless, glutamate does not seem to be responsible for cellular death in our study, given the absence of cell death that was found in our experimental conditions.
As a whole, our findings suggest that ODLG predisposes cortical neurons to cellular vulnerability and could resemble some neurotoxic mechanisms within the penumbra of ischemic rats and humans. In these conditions, cells are able to survive by inducing compensatory mechanisms that reduce neurodegeneration. The relevance of our findings is its potential to prevent cell death and repair damaged neurons in cerebral ischemia. The lack of O2 and low glucose could predispose neurons to vulnerable conditions as in the penumbral area, through ROS production. Nonetheless, cells are capable of surviving through compensatory defense/protective mechanisms under these vulnerable conditions (antioxidant defenses). However, part of these mechanisms could be lost at reperfusion, mainly as a consequence of mitochondrial membrane alteration under hypoxia. Cells under hypoxia could activate endogenous antioxidant mechanisms to ameliorate cell death and compensate for mitochondrial membrane imbalances . Thus, the use of antioxidants does not seem to protect neurons during reperfusion because there was a reversion of ROS formation during this period. During induced ODLG, neurons are able to activate endogenous antioxidant responses. Thus, the use of cellular and mitochondrial membrane protectors may be a good way to protect neurons during reperfusion after ischemia.
4. Experimental Section
4.1. Cell Isolation and Culture
Brains from fetal (E19) rats of 19 days gestation were used. Brain neurons were obtained according to the procedure described by Segal  with minor modifications. Isolated neurons were suspended in EMEM medium with addition of 0.3 g/L glutamine, 3 g/L glucose, 10% FCS, 100 U/mL penicillin and 100 μg/mL streptomycin. Cells, at a density of 106 cells/cm well, were placed on plastic Petri dishes treated with 10 μg/mL of poly-d-lysine, to attach them to the plates. Cells were then incubated in a humidified incubator with 5% CO2/95% air at 37 °C. After 72 h, the incubation medium was replaced with a fresh medium containing 10 μM of cytosine arabinoside to prevent glial overgrowth in the culture medium. Cells were studied after seven days “in vitro” (7 DIV). Cell purity was checked by staining cells both with cresyl violet to identify neurons and anti-GFAP antibody to identify atrocytes.
Glial contamination was tested following the procedure from Figueroa et al. .
4.2. ODLG Treatment
All experiments were performed at seven days of culture. The cultured medium was removed and replaced by an EMEM commercial medium containing 1 g/L glucose and 10% of fetal calf serum (low glucose). This treatment was performed on two sets of cells. Cells were placed for indicated time, in a chamber at 37 °C within an atmosphere of 95% N2/5% CO2 (O2 deprivation). After different times of ODLG, a set of cells was taken and several biochemical markers were assayed.
Parallel control experiments were performed. In this case, the neurons were cultured with commercial EMEM medium plus 3 g/L of glucose under normal atmosphere (95% air/5% CO2). Thus, the controls were not under ODLG.
After cells were subjected to ODLG for several periods of time (1, 3, 5, 12, 24 and 48 h), the medium was removed and replaced by normal medium (medium with serum plus antibiotics containing 3 g/L glucose plus 0.3 g/L glutamine). After this, cells were placed for 24 h, in a cell incubator containing 95% air/5% CO2 and 37 °C. At the end of this protocol, all parameters were evaluated for each experimental condition.
4.4. Assessment of Cell Viability
Cell viability was tested by crystal violet and the XTT assay.
4.4.1. Crystal Violet Determination
Cortical neurons were washed twice with PBS (8.1 mM Na2HPO4, 2.7 mM KH2PO4, 173 mM NaCl, pH 7.4) and then exposed to 0.2% crystal violet in 2% ethanol for 20 min. After this time, cells were washed with distilled water until the excess dye was removed and then were lysed by adding 1% sodium dodecyl sulfate (SDS). Finally, absorbance was measured at 560 nm.
4.4.2. XTT Determination
This assay is based on the ability of live metabolically active cells to reduce yellow tetrazolium salt (XTT) to form an orange formazan dye. Thus, this conversion can only occur in living cells. The newly-formed formazan dye is directly quantified using a scanning multi-well spectrophotometer at a wavelength of 492 nm (reference wavelength 690). The amount of orange formazan formed, as monitored by the absorbance, directly correlates to the number of living cells. Control and treated neurons were washed with PBS and incubated with the XTT solution (final concentration 0.3 mg/mL) according to Kit specifications. After this incubation period, orange dye solution was spectrophotometrically quantified at a wavelength of 492 nm (reference wavelength 690 nm). Results were expressed as percentages as compared to control cells, which were considered as 100%.
4.5. Measurement of ROS Formation
To assay ROS formation, 2,7-dichlorodihydrofluorescein diacetate (H2DCF-DA), a non-fluorescent lipophilic reagent, was used. H2DCF-DA enters the cells, where it is transformed into 2,7-dichlorodihydrofluorescein (H2DCF) by the action of intracellular stearases. H2DCF is oxidized to fluorescent DCF by hydrogen peroxide. H2DCF-DA (5 μM) was added to the cells, before subjecting to different ODLG conditions. After each treatment, the incubation medium was removed and the cells were washed twice with PBS. Finally, fluorescence was measured in an FL600-BioTek spectrofluorometer (Winooski, VT, USA) with filters of 485/20 nm excitation and 530/25 nm emission. Results are expressed as arbitrary fluorescence units (AFU).
4.6. Lactate Dehydrogenase (LDH) Release
For LDH determination, the culture media from the control and experimental cultures treatments were collected and the neurons lysed by adding 0.1 M Tris-HCl (pH 7.4), containing 0.1% Triton X-100, and then centrifuged at 13,000 rpm using an Eppendorf centrifuge. LDH activity was measured in culture medium as well as in the cells according to López et al. . Activity of LDH release is given as a percentage compared to the total LDH content (LDH in the supernatant + LDH inside the cells).
4.7. Caspase-3 Activity Measurement
Control and treated cortical neurons were washed with PBS and lysed with cell lysis buffer (10 mM Tris-HCl, 10 mM NaH2PO4/Na2HPO4, pH 7.5, 130 mM NaCl, 0.5% Triton X-100, 10 mM Na4P2O7 and 2 mM dithiothreitol (DTT). Lysates were centrifuged at 13,000× g for 5 min. Caspase-3 activity was measured in the supernatants. Supernatants were incubated at 37 °C for 2–4 h in caspase-3 assay buffer (20 mM HEPES, pH 7.5, 10% glycerol, 2 mM DTT containing 20 μM Ac. N-acetyl-Asp-Glu-Val-Asp-(7-amino-4-methylcoumarin (AcDEVD-AMC). The fluorogenic 7-amino-methylcoumarin (AMC) liberated from Ac-DEVD-AMC was monitored using a spectrofluorometer Bio-Tek FL 600, at excitation wavelength of 360/20 nm and an emission wavelength range 460/20. Enzymatic activity is expressed as arbitrary fluorescence unit after 2 h per μg protein (AFU/2 h/μg protein). The amount of proteins in lysed cells was monitored by Bradford .
4.8. Cytochrome Oxidase Activity
After each treatment, the incubation medium was removed and cells were washed with PBS and lysed with 200 μL of 0.1 M potassium phosphate buffer pH 7.5 which contained 0.5% Triton X-100. The lysed cells were centrifuged at 13,000 rpm for 5 min before collecting supernatants. Reduced cytochrome c (7 mg) was dissolved in 1 mL of 0.1 M of potassium phosphate buffer pH 7.5 and dithionite was added to ensure cytochrome reduction. Excess dithionite was removed by passing the cytochrome c solution through a Sephadex G-25 column equilibrated with the buffer (Amersham Bioscience, Arlington, MA, USA). The eluyent was taken and adjusted to an optic density of 0.7 absorbance. The extract was added to 1 mL of this solution and absorbance measured at 550 nm. Activity was expressed as OD/10 min/mg protein.
4.9. Measurement of Glutathione
After treatments, the cultured medium was removed and cells washed with PBS. The cells were placed under ice and 300 μL of 0.1 M of sodium phosphate-EDTA pH = 8 and 100 μL of 25% phosphoric acid were added to each well. The cell suspension was centrifuged at 13,000× g for 5 min and the supernatant was taken. Glutathione concentration was expressed as AFU/μg protein. Reduced glutathione was evaluated following the protocol from Hissin and Hilf .
4.10. Measurement of Amino Acid Secretion
HPLC analysis of amino acids was performed following a procedure from Márquez et al. . The cellular medium was removed and cells were washed twice with PBS. Cells were stimulated during 15 min at 37 °C with 0.5 mL of fresh Locke medium containing 60 mM KCl. After stimulation, the solution was taken and the amino acids in the solution were dansylated with dansyl chloride. Separation of dansyl-derivates was carried out in a 5 μM Spherisorb-ODS-2 column (15 × 0.46 cm; Sigma Aldrich, St. Louis, MO, USA) using a reversed-phase high-performance liquid chromatography with UV detection at 254 nm. Peaks were integrated using a Spectraphysic integrator (Sigma Aldrich) and quantified by comparison with simultaneously-prepared amino acid standards. Cells were lysed by adding 0.5 mL distilled water. The lysed cells were centrifuged at 13,000 rpm in an Eppendorf centrifuge (Hamburg, Germany) for 5 min and the supernatants were collected and proteins were measured. The amount of protein in the lysed cells was quantified using the Bradford assay . Results were expressed as nmols of neurotransmitter/mg protein.
4.11. Membrane Potential Measurement
Changes in the membrane potential of neurons were monitored with the fluorescent dye bisoxonol (bis-[1,3-diethyl-thio-barbiturate]-trimethineoxonol), according to the Waggonet method . The control neurons, and neurons after treatment were washed and incubated with 0.2 μM bisoxonol for 30 min. After this treatment, bisoxonol was removed and the cells were washed with PBS and suspended in PBS. Finally, fluorescence was measured at wavelengths of 540 nm excitation and 565 nm emission, and monitored with a FL600-BioTek spectrofluorimeter Fluorescence (Winooski, VT, USA) intensity was reported as arbitrary fluorescence units.
4.12. Mitochondrial Membrane Potential Assay
Mitochondrial membrane potential was measured following the protocol by Tenneti et al., , with minor modifications. Control and treated cells were washed with PBS and incubated for 30 min with 500 nM of tetramethylrhodamine methyl ester (TMRM) and dissolved in Locke medium (140 mM NaCl, 4.4 mM KCl, 2.5 mM CaCl2, 1.2 mM MgSO4, 1.2 mM KH2PO4, 4 mM NaHCO3, 5.5 mM glucose and 10 mM HEPES, adjusted to pH 7.5). Finally, cells were washed with PBS, and the fluorescence was measured using a FL600-BioTek spectrofluorimeter at 530/25 nm exc. and 590/20 nm em.
4.13. Analysis of Gene Expression
Total RNA was isolated from 5 × 106 cells of primary neuron cultures, using a RNase mini kit from Qiagen, Hilden, Germany) following the manufacturer’s instructions with the optional RNase-free DNase step to avoid contamination with genomic DNA. RNA concentration was determined by spectrophotometer, reading absorbance at 260 nm and defining one optical density unit as equivalent to 40 μg/mL. The ratio between the absorbance values at 260 and 280 nm gave an estimation of RNA purity.
4.13.1. RT-PCR Analysis
RNasy Mini Kit (Qiagen, Valencia, CA, USA) was used for total RNA isolation. Reverse transcription (RT) was carried out for 1 h at 55 °C with oligodeoxythymidylate primer using 5 μg of total RNA from each sample for complementary DNA synthesis.
Real time quantitative PCR to determine the levels of rat HIF1, HIF3, SOD1, GPX3 and housekeeping GAPDH mRNAs were performed using specific primers (See Table 1) synthesized at Sigma-Genosys (Oakville, ON, Canada).
4.13.2. Real-Time PCR
The SYBR Green PCR Master Mix (Applied Biosystems, and the 7900 HT Fast Real-Time PCR System (Applied Biosystems, Foster City, CA, USA) were used to detect the real-time quantitative PCR products of reverse-transcribed cDNA samples, according to the manufacturer’s instructions. q-PCR conditions used are as follows: 95 °C (10 min), 40 cycles of 15 s at 95 °C and annealing for 1 min at 60 °C. Two independent quantitative PCR assays were performed for each gene and measured in triplicate. Two non-template controls were run for each quantitative PCR assay, and genomic DNA contamination of total RNA minus controls (samples without the reverse transcriptase).
4.14. Statistical Analysis
Data are presented as means ± SEM of three/four independent experiments using different cell cultures, each one performed in triplicate with different batches of cells. Statistical comparisons between two or more populations were made using the ANOVA on rank test to evaluate the normality and variance of the data. If both parameters are confirmed then the Holme-Sidak test detects significant differences between groups. When one of these parameters is absent, we did a Kruskal-Wallis non-parametric analysis as well as Dunn’s pos Hoc test using the SigmaPlot 11.0 software (Systat Software, Inc., San Jose, CA, USA).
4.15. Ethics Statement
Pregnant rats were obtained from the “Laboratory Animal form the Universidad Complutense of Madrid (U.C.M)”; License number #ES280790000086. The work was also approved by the University Animal Care Committee (C.E.A = Committee of Experimental Research and Ethics) from Universidad Complutense de Madrid (U.C.M); form number RD # 53/2013 for research and it was carried out in strict accordance with Guidelines for the Care and Use of Laboratory (European Council Directive 86/609/EEC). All surgery was performed under sodium pentobarbital anesthesia, and all efforts were made to minimize suffering of animals.
The major points of the investigation presented here may be stated as follows: (1) Cortical neurons subjected to ODLG conditions (1–5 h) do not die but remain in lethargic stage. This condition protects neurons by saving energy and nutrients; (2) During this ODLG time cortical neurons showed protective mechanisms in their upregulation of HIF-1α and HIF-3α production as well as of antioxidant enzymes (reduced glutathione, SOD-1 and GPX3), which could help cells recover during reperfusion; and (3) After long ODLG times (12–24 h), cortical neurons are under the same conditions as those at shorter ODLG times, but during this longer period there is cell damage and mitochondrial membrane alterations which do not allow recovery during reperfusion. Taken together, these molecular events in our ODLG model are in accordance with some molecular aspects reported within the penumbra of ischemic rats . Consequently, drugs that can induce HIF-1 and SOD-1 could helpful to recover after short periods of ischemia.
This study was supported by grants from Ministerio de Ciencia e Innovacion (MICINN) (SAF2010-20337) and UCM-Santander (GR35/10-B) and Cienporciennatural ( http://www.cienporciennatural.com). We thank Carol Fox Warren and Mikel Erdocia for revising the manuscript.
Conflicts of Interest
The authors declare no conflict of interest. Cienporciennatural Company declare no conflict of interest.
- Lo, E.H.; Dalkara, T.; Moskowitz, M.A. Mechanism, challenges and opportunities in stroke. Nat. Rev. Neurosci 2003, 4, 399–405. [Google Scholar]
- Jie, L.; Yuqin, C.; Yao, D.; Shuai, H.; Yuanyuan, W. Occlusion of middle cerebral artery induces apoptosis of cerebellar cortex neural cells via caspase-3 in rats. Turk. Neurosurg 2011, 21, 567–574. [Google Scholar]
- Northington, F.J.; Chavez-Valdez, R.; Martin, L.J. Neuronal cell death in neonatal hypoxia-ischemia. Ann. Neurol 2011, 69, 743–758. [Google Scholar]
- Choi, S.Y.; Lee-Kwon, W.; Lee, H.H.; Lee, J.H.; Sanada, S.; Kwon, H.M. Multiple cell death pathways are independently activated by lethal hypertonicity in renal epithelial cells. Am. J. Physiol. Cell Physiol 2013, 305, C1011–C1020. [Google Scholar]
- Benveniste, H.; Drejer, J.; Schousboe, A.; Diemer, N.H. Elevation of the extracellular concentration of glutamate and aspartate in rat hippocampus during transient cerebral ischemia monitored by intracerebral microdyalisis. J. Neurochem 1984, 43, 1369–1374. [Google Scholar]
- Chan, P.H. Oxigen radicals in focal cerebral ischaemia. Brain Pathol 1994, 4, 59–65. [Google Scholar]
- Chan, P.H. Reactive oxygen radicals in signalling and damage in the ischemic brain. J. Cereb. Blood Flow Metab 2001, 21, 2–14. [Google Scholar]
- Kotur-Stevuljevic, J.; Memon, L.; Stefanovic, A.; Spasic, S.; Spasojevic-Kalimanovska, V.; Bogavac-Stanojevic, N.; Kalimanovska-Ostric, D.; Jelić-Ivanovic, Z.; Zunic, G. Correlation of oxidative stress parameters and inflamatory moukers in coronary arteric disease patients. Clin. Biochem 2007, 40, 181–187. [Google Scholar]
- Nistico, R.; Piccirilli, S.; Cucchiaroni, M.L.; Armogida, M.; Guatteo, E.; Giampa, C.; Fusco, F.R.; Bernardi, G.; Nistico, G.; Mercuri, N.B. Neuroprotective effect of hydrogen peroxide on an in vitro model of brain ischaemia. Br. J. Pharmacol 2008, 153, 1022–1029. [Google Scholar]
- Allen, R.G.; Tresini, M. Oxidative stress and gene regulation. Free Radic. Biol. Med 2000, 28, 463–499. [Google Scholar]
- Ten, V.S.; Starkovy, A. Hypoxic-ischemic injury in the developing brain: The role of reactive oxigen species originaty in mitochondria. Neurol. Res. Int 2012. [Google Scholar] [CrossRef]
- Rothman, S. Synaptic release of excitatory amino acid neurotransmitter mediated anoxic neuronal death. J. Neurosci 1984, 4, 1884–1891. [Google Scholar]
- Sen, C.K.; Packer, L. Antioxidant and redox regulation of gene transcription. FASEB J 1996, 10, 709–720. [Google Scholar]
- Finkel, T. Oxidant signals and oxidative stress. Curr. Opin. Cell Biol 2003, 15, 247–254. [Google Scholar]
- Rhee, S.G.; Yang, K.S.; Kang, S.W.; Woo, H.A.; Chang, T.S. Controlled elimination of intracellular H2O2: Regulation of peroxiredoxin, catalase, and glutathione peroxidase via post-translational modification. Antioxid. Redox Signal 2005, 7, 619–626. [Google Scholar]
- Louzada-Junior, P.; Dias, J.J.; Santos, W.F.; Lachat, J.J.; Bradford, M.F.; Coutinho-Netto, J. Gutamate release in experimental ischemia of the retina: An approach using microdialisis. J. Neurochem 1992, 59, 358–363. [Google Scholar]
- Ankarcrona, M. Glutamate induces cellular death: Apoptosis or necrosis? Prog. Brain Res 1998, 116, 265–272. [Google Scholar]
- Castellanos, M.; Sobrino, T.; Pedraza, S.; Moldes, O.; Pumar, J.M.; Silva, Y.; Serena, J.; Garcia-Gil, M.; Castillo, J.; Dávalos, A. High plasma glutamate concentrations are associated with infarct growth in acute ischemic stroke. Neurology 2008, 71, 1862–1868. [Google Scholar]
- Antonelli, T.; Tomasini, M.C.; Fournier, J.; Mazza, R.; Tanganelli, S.; Pirondi, S.; Fuxe, K.; Ferraro, L. Neurotensin receptor involvement in the rise of extracellular glutamate levels and apoptotic nerve cell death in primary cortical culture after oxygen and glucose deprivation. Cereb. Cortex 2008, 18, 1748–1757. [Google Scholar]
- Chi, O.Z.; Hunter, C.; Liu, X.; Weiss, H.R. Effect of exogenous excitatory amino acid neurotransmitters on blood-brain barrier disruption in focal cerebral ischemia. Neurochem. Res 2009, 34, 1249–1254. [Google Scholar]
- Pak, E.; Lee, G.J.; Choi, S.; Choi, S.K.; Kang, S.W.; Pak, K.J.; Pak, H.K. The role of glutamate releae on voltage-dependent anion channels (VDAC) mediated apoptosis in a eleven vessel occlusion model in rats. PLoS One 2010, 5, e15192. [Google Scholar]
- Sun, C.; Merg, Q.; Zhang, L.; Wang, H.; Quirion, R.; Zheng, W. Glutamate alterates IGF-1 receptor tyrosine phosphorilation in mouse brain: Possible significance in ischemic brain damage. Neurosci. Res 2012, 74, 290–297. [Google Scholar]
- Wang, D.; Zhao, Y.; Zhang, Y.; Zhang, T.; Shang, X.; Wan, J.; Liu, Y.; Kong, Q.; Sun, B.; Mu, L.; et al. Hypotermia protects against oxygen-glucose deprivation induced neuronal injury by downregulating the reverse transport of glutamate by astrocytes as mediated by neurons. Neuroscience 2013, 237, 130–138. [Google Scholar]
- Bao, D.Z.; Bao, H.Y.; Yao, L.Z.; Pan, Y.G.; Zhu, X.R.; Yang, X.S.; Wang, H.; Huang, Y.N. 64-Slice spiral CT perfusion combined with vascular imaging of acute ischemic stroke for assessment of infarct core and penumbra. Exp. Ther. Med 2013, 6, 133–139. [Google Scholar]
- Heiss, W.D.; Graf, R. The ischemic penumbra. Curr. Opin. Neurol 1994, 7, 11–19. [Google Scholar]
- Ginsberg, M.D. The new language of cerebral ischemia. Am. J. Neuroradiol 1997, 18, 1435–1445. [Google Scholar]
- Pulsinelli, W.A.; Jacewicz, M.; Levy, D.E.; Petito, C.K.; Plum, F. Ischemic brain injury and the therapeutic window. Ann. N. Y. Acad. Sci 1997, 835, 187–193. [Google Scholar]
- Siddiq, A.; Ayoub, A.; Chavez, J.C.; Aminova, L.; Shah, S.; LaManna, J.C.; Patton, S.M.; Connor, J.R.; Cherny, R.A.; Volitakis, I.; et al. Hypoxia-inducible factor prolyl 4-hydroxulase inhibition. A target for neuroprotection in the central nervous system. J. Biol. Chem 2005, 280, 41732–41743. [Google Scholar]
- Semenza, G.L.; Roth, P.H.; Frang, H.M.; Wang, G.L. Transcriptional regulation of genes encoding glycolitic enzymes by hypoxia-inducible factor. J. Biol. Chem 1994, 269, 23757–23763. [Google Scholar]
- Baba, K.; Muraguchi, T.; Imaoka, S. Role of the hypoxia response pathway in lens formation during embryonic development of Xenopus laevis. FEBS Open Bio 2013, 3, 490–495. [Google Scholar]
- Zhao, Y.; Matsuo-Takasaki, M.; Tsuboi, I.; Kimura, K.; Salazar, G.; Yamashita, T.; Ohneda, O. Dual functions of hypoxia inducible factor-1 alpha for the commitment of mouse embryonic stem cells toward a neural lineage. Stem Cells Dev 2013. [Google Scholar] [CrossRef]
- Semenza, G.L. Oxygen sensing, hypoxia-inducible factors, and disease pathophysiology. Annu. Rev. Pathol 2013. [Google Scholar] [CrossRef]
- Semenza, G.L. Hypoxia-inducible factors in physiology and medicine. Cell 2012, 148, 399–408. [Google Scholar]
- Semenza, G.L. Hypoxia-inducible factor 1: Oxygen homeostasis and disease pathophysiology. Trends Mol. Med 2001, 7, 345–350. [Google Scholar]
- Segal, M. Rat hippocampus neurons in culture: Responses to electrical and chemical stimuli. J. Neurophysiol 1983, 50, 1249–1264. [Google Scholar]
- Figueroa, S.; Oset-Gasque, M.J.; Arce, C.; Martinez-Honduvilla, C.J.; González, M.P. Mitochondrial involvement in nitric oxide-induced cellular death in cortical neurons in culture. J. Neurosci. Res 2006, 83, 441–449. [Google Scholar]
- Ebert, B.L.; Bunn, H.F. Regulation of transcription by hypoxia requires a multiprotein complex that induces hypoxia-inducible factot 1, an adjacent transcription factor, and p300/CREB-binding protein. Mol. Cell Biol 1998, 18, 4089–4096. [Google Scholar]
- Siddqi, A.; Aminova, L.R.; Ratan, R.R. Hypoxia inducible factor prolyl 4-hydroxylase encimes: Center stage in the battle against hypoxia, metabolic compromise and oxidative stress. Neurochem. Res 2007, 32, 931–946. [Google Scholar]
- Wu, C.; Hu, Q.; Chen, J.; Yan, F.; Li, J.; Wang, L.; Mo, H.; Gu, C.; Zhang, P.; Chen, G. Inhibiting HIF-1α by 2ME2 ameliorates early brain injury after experimental subarachnoid haemorrhage in rats. Biochem. Biophys. Res. Commun 2013, 437, 469–474. [Google Scholar]
- Chen, X.; Guan, T.; Li, C.; Shang, H.; Cui, L.; Li, X.M.; Kong, J. SOD1 aggregation in astrocytes following ischemia/reperfusion injury: A role of NO-mediated S-nitrosylation of protein disulfide isomerase (PDI). J. Neuroinflamm 2012, 237, 1–14. [Google Scholar]
- Kim, W.; Kim, D.W.; Yoo, D.Y.; Chung, J.Y.; Hwang, I.K.; Won, M.H.; Choi, S.Y.; Jeon, S.W.; Jeong, J.H.; Hwang, H.S.; et al. Neuroprotective effects of PEP-1-Cu,Zn-SOD against ischemic neuronal damage in i.e., rabbit spinal cord. Neurochem. Res 2012, 37, 307–313. [Google Scholar]
- Klimova, T.; Chandel, N.S. Mitochondrial complex III regulates hypoxic activation of HIF. Cell Death Differ 2008, 15, 660–666. [Google Scholar]
- Livnat, A.; Barbiro-Michaely, E.; Mayevsky, A. Mitochondrial function and cerebral blood flow variable responses to middle cerebral artery occlusion. J. Neurosci. Methods 2010, 188, 76–82. [Google Scholar]
- Jones, N.M.; Bergeron, M. Hypoxic preconditioning induces changes in HIF-1 target gene in neonatal rat brain. J. Cereb. Blood Flow Metab 2001, 21, 1105–1114. [Google Scholar]
- Schaller, S.; Graf, R. Cerebral ischemic preconditioning. An experimental phenomenon or a clinical important entity of stroke prevention? J. Neurol 2002, 249, 1503–1511. [Google Scholar]
- Xia, D.Y.; Li, W.; Qian, H.R.; Yao, S.; Liu, J.G.; Qi, X.K. Ischemia preconditioning is neuroprotective in a rat cerebral ischemic injury model through autophagy activation and apoptosis inhibition. Braz. J. Med. Biol. Res 2013, 46, 580–588. [Google Scholar]
- Mattson, M.P.; Culmsec, C.; Yu, Z.F. Apoptotic and antiapoptotic mechanisms in stroke. Cell Tissue Res 2000, 301, 173–187. [Google Scholar]
- Levenbrown, Y.; Ashraf, Q.M.; Maounis, N.; Mishra, O.P.; Delivoria-Papadopoulos, M. Phosphorylation of caspase-9 in the cytosolic fraction of the cerebral cortex of newborn piglets following hypoxia. Neurosci. Lett 2008, 447, 96–99. [Google Scholar]
- Yager, J.Y.; Kala, G.; Hertz, L.; Juurlink, B.H. Correlation between content of high-energy phosphates and hypoxic-ischemic damage in immature and mature astrocytes. Brain Res. Dev 1994, 82, 62–68. [Google Scholar]
- Arce, C.; Arteaga, J.L.; Sánchez-Mendoza, E.; Oset-Gasque, M.J.; Cañadas, S.; González, M.P. Added after anoxia-reoxigenation stress, genistein rescues from death the rat embryo cortical. Neurosci. Med 2010, 1, 50–59. [Google Scholar]
- Zhang, X.; Yan, H.; Yuan, Y.; Gao, J.; Shen, Z.; Cheng, Y.; Shen, Y.; Wang, R.R.; Wang, X.; Hu, W.W.; et al. Cerebral ischemia-reperfusion-induced autophagy protects against neuronal injury by mitochondrial clearance. Autophagy 2013, 9, 1321–1333. [Google Scholar]
- López, E.; Figueroa, S.; Oset-Gasque, M.J.; González, M.P. Apoptosis and necrosis: Two distinct events induced by cadmium in cortical neurons in culture. Br. J. Pharmacol 2003, 138, 901–911. [Google Scholar]
- Bradford, M.A. Rapid sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal. Biochem 1976, 72, 248–253. [Google Scholar]
- Hissin, P.J.; Hilf, R. A fluorometric method for determination of oxidized and reduced glutathione in tissues. Anal. Biochem 1976, 74, 214–226. [Google Scholar]
- Marquez, F.J.; Quesada, A.R.; Sanchez-Jimenez, F.; de Castro, Y.N. Determination of 27 dansyl amino acid derivates in biological fluids by reversed-phase high-performance liquid chromatography. J. Chromatogr 1986, 380, 275–283. [Google Scholar]
- Waggoner, A.S. Dye indicators of membrane potential. Ann. Rev. Biophys. Bioenerg 1979, 8, 47–68. [Google Scholar]
- Tenneti, L.; D’Emilia, D.M.; Troy, C.M.; Lipton, S.A. Role of caspase in N-methyl-d-Aspartate-induced apoptosis in cerebrocortical neurons. J. Neurochem 1998, 71, 946–959. [Google Scholar]
- Bonova, P.; Burda, J.; Danielisova, V.; Nemethova, M.; Gottlieb, M. Development of a pattern in biochemical parameters in the core and penumbra during infarct evolution after transient MCAO in rats. Neurochem. Int 2013, 62, 8–14. [Google Scholar]
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