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Molecular Medicine

, Volume 13, Issue 7–8, pp 344–349 | Cite as

Zinc Inhibits Astrocyte Glutamate Uptake by Activation of Poly(ADP-ribose) Polymerase-1

  • Sang Won Suh
  • Koji Aoyama
  • Conrad C. Alano
  • Christopher M. Anderson
  • Aaron M. Hamby
  • Raymond A. Swanson
Open Access
Proceedings

Abstract

Several processes by which astrocytes protect neurons during ischemia are now well established. However, less is known about how neurons themselves may influence these processes. Neurons release zinc (Zn2+) from presynaptic terminals during ischemia, seizure, head trauma, and hypoglycemia, and modulate postsynaptic neuronal function. Peak extracellular zinc may reach concentrations as high as 400 µM. Excessive levels of free, ionic zinc can initiate DNA damage and the subsequent activation of poly(ADP-ribose) polymerase 1 (PARP-1), which in turn lead to NAD+ and ATP depletion when DNA damage is extensive. In this study, cultured cortical astrocytes were used to explore the effects of zinc on astrocyte glutamate uptake, an energy-dependent process that is critical for neuron survival. Astrocytes incubated with 100 or 400 µM of zinc for 30 min showed significant decreases in ATP levels and glutamate uptake capacity. These changes were prevented by the PARP inhibitors benzamide or DPQ (3,4-dihydro-5-(4-(1-piperidinyl)butoxyl)-1(2H)-isoquinolinone) or PARP-1 gene deletion (PARP-1 KO). These findings suggest that release of Zn2+ from neurons during brain insults could induce PARP-1 activation in astrocytes, leading to impaired glutamate uptake and exacerbation of neuronal injury.

Introduction

Astrocytes perform several functions that are essential for normal neuron activity, including glutamate uptake, K+ and H+ buffering, water transport, and metabolite exchange (1,2). These astrocyte functions can also influence neuronal survival during ischemia and other brain insults (2). Glutamate homeostasis is a key aspect of astrocyte-neuron interaction during ischemia because of the sensitivity of many neurons to glutamate excitotoxicity (3). Microdialysis studies indicate that extracellular glutamate is maintained at low concentrations in the (viable) ischemic penumbra (4), and failure of astrocyte glutamate uptake may trigger the conversion of ischemic but viable tissue to infarction (5,6). Astrocyte glutamate uptake is accomplished by Na+-dependent transporters (7,8). These transporters move glutamate into astrocytes against a steep concentration gradient by coupling glutamate translocation to the transmembrane Na+, K+, and voltage gradients. These gradients are in turn maintained by membrane Na+/K+ ATPase activity, such that glutamate uptake is ultimately ATP dependent.

While the importance of glutamate uptake and other astrocyte processes is well established, little is known about how neurons themselves may affect this process. The present study explores a mechanism by which neurons may activate astrocyte poly(ADP-ribose) polymerase 1 (PARP-1), thus impairing energy metabolism and glutamate uptake in these cells. PARP activity is shared by a family of enzymes, of which PARP-1 is the most abundant and well characterized (9,10). When activated by DNA strand breaks or kinks, PARP-1 consumes NAD+ to form poly(ADP-ribose) polymers on several acceptor proteins, including histones, DNA polymerase, and DNA ligases (9,11,12). This process appears to facilitate DNA repair; however, excessive PARP-1 activation results in NAD+ and ATP depletion when DNA damage is extensive (10,13,14). Because glutamate uptake requires ATP, it follows that extensive PARP-1 activation in astrocytes could impair glutamate uptake.

Zinc (as Zn2+) leads to PARP-1 activation, probably as a result of increased production of reactive oxygen species in the presence of elevated Zn2+ (15, 16, 17, 18, 19). Neurons release Zn2+ from presynaptic terminals during pathological conditions such as ischemia, seizure, brain trauma, and hypoglycemia (20, 21, 22, 23, 24, 25, 26, 27). In those conditions extracellular Zn2+ concentration may reach 100–400 µM (28, 29, 30, 31, 32), although direct measurements of brain extracellular Zn2+ have not confirmed elevations to this level (33).

The present study examines the effect of Zn2+ elevations on ATP levels and glutamate uptake in cultured astrocytes. We show that Zn2+ can inhibit glutamate uptake in mouse cortical astrocytes by PARP-1 activation and subsequent ATP depletion, and that this effect is attenuated by the PARP inhibitors benzamide or DPQ (3,4-dihydro-5-[4-(1-piperidinyl) butoxyl]-1(2H)-isoquinolinone) and by PARP-1 gene deficiency.

Methods and Materials

The studies were performed in accordance with protocols approved by the animal studies committee of the San Francisco Veterans Affairs Medical Center. Reagents were purchased from Sigma Chemical Co (St. Louis, MO, USA) except where noted.

Cell cultures

Wild-type astrocyte cultures were prepared from cortices of one-day-old Swiss-Webster mice (Simonsen, Gilroy, CA, USA) as described previously (34,35) and plated into 24-well Falcon culture plates. The PARP-1−/− mice were the 129S Adprt1tm1Zqw strain obtained from Jackson Laboratory (Bar Harbor, ME, USA) and originally developed by Wang et al. (36). The wild-type and PARP-1−/− cortices were harvested, freed of meninges, dissociated with papain digestion (with DNase) and subsequent trituration, and plated on 24-well Falcon culture plates or glass coverslips. Cells were treated for 48 h with 20 µM cytosine arabinoside at confluence (12–15 d in vitro) to prevent microglial proliferation. This medium was replaced with Eagle’s minimal essential medium containing 5 mM glucose supplemented with 5% fetal bovine serum (HyClone, Logan, UT, USA), 2mM glutamine, 100 nM sodium selenate, and 200 nM ±-tocopherol. The astrocyte cultures were used, when confluent, at 20 to 30 d in vitro (37).

Experimental procedures

Experiments were initiated by replacing the culture medium with artificial cerebrospinal fluid (ACSF). The ACSF contained (in mM) KCl, 3.1; NaCl, 134; CaCl2, 1.2; MgSO4, 1.2; KH2PO4, 0.25; NaHCO3, 15.7; and glucose, 2. The pH was adjusted to 7.2 while the solution was equilibrated with 5% CO2 at 37 °C. Osmolarity was verified at 290–310 mOsm with a Wescor vapor pressure osmometer (Logan, UT, USA). Zinc and PARP inhibitors were added from concentrated stocks prepared in ACSF immediately before use and adjusted to pH 7.2 when necessary. An exposure to Zn2+ (ZnCl2) was performed at 37 °C in a 5% CO2 atmosphere. Thirty minutes of exposure to 100 or 400 µM Zn2+ (as ZnCl2) was performed in ACSF. After the exposure, cultures were washed two times with ACSF and were placed back into the incubator. When used, 1 mM of benzamide or 25 µM of DPQ was added to the medium one hour before and during the Zn2+ exposure. Cultures were then maintained in ACSF until biochemical studies were performed.

ATP assay

For ATP assays, cells were lysed in boiling buffer containing 100 mM Tris and 4 mM EDTA, pH 7.75. Fifty milliliters of cell lysates were mixed with 50-mL aliquots of luciferase/luciferin mixture provided with an ATP bioluminescence assay kit (Roche Diagnostics GmbH, Mannheim, Germany), and photon emission was detected with a luminometer. ATP concentrations were calibrated against ATP standards and expressed as nanomoles per milligram of protein.

Glutamate uptake

Glutamate uptake was measured as described previously (38) with minor modifications. Assays were initiated by replacing the culture medium with ACSF. After a 20-min preincubation in this medium, each culture well received 1.67 µCi/mL L-[14C(U)]glutamate plus unlabeled glutamate to achieve a total glutamate concentration of 100 µM. Uptake was terminated after a 7-min incubation at 37 °C by two washes in ice-cold Hank’s balanced salt solution, followed immediately by cell lysis in 0.1N NaOH. Aliquots were divided for scintillation counting and protein determinations.

Cell death determinations

Astrocyte death was quantified by measuring lactate dehydrogenase (LDH) activity in cell lysates harvested 24 h after Zn2+ exposures. Percentage cell death was calculated by normalizing the LDH values to LDH activity measured in lysates from control (wash only) culture wells (38,39).

Statistical analyses

All data are presented as means ± SEM and were assessed by analysis of variance (ANOVA) followed by the Bonferroni multiple comparisons test, as post-hoc comparison, for differences between selected pairs of groups. P values less than 0.05 were considered statistically significant.

Results

Zn2+ Inhibits Uptake of Glutamate into Cultured Mouse Astrocytes

The basal rate of L-[14C]glutamate uptake in wild-type primary mouse cortical astrocyte cultures was 8.08 ± 0.35 nmol/min/mg protein. Astrocytes incubated with Zn2+ (100–400 µM) for 30 min exhibited delayed and dose-dependent reductions in glutamate uptake that became more pronounced with progressive time after zinc exposure and washout (Figure 1). Studies performed with 10 uM Zn2+ added to the medium showed no effect on glutamate uptake (not shown).
Figure 1

Zn2+ impairs astrocyte glutamate uptake in a dose- and time-dependent manner. Astrocytes were exposed for 30 min to Zn2+ at the designated concentrations, and glutamate uptake was assessed immediately (zero hours), one hour, or three hours after zinc removal. Data points are means of three to four independent experiments (n = 3-4), each with measurements from two to three culture wells. *P< 0.05 versus control at the designated time point.

PARP Inhibitors and PARP-1 Gene Deletion Prevent Zn2+-Induced Astrocyte Glutamate Uptake Inhibition

As shown in Figure 2A and 2B, astrocytes incubated with Zn2+ showed reduced glutamate uptake at one hour after Zn2+ washout, and this reduction was significantly prevented in cultures treated with benzamide (1 mM) or DPQ (25 µM). Zinc-induced glutamate uptake inhibition was also attenuated in astrocytes prepared from PARP-1−/− mice, further suggesting that the effect of Zn2+ on glutamate uptake is mediated by PARP-1 activation (Figure 2C).
Figure 2

PARP inhibitors and PARP-1 gene deletion prevent Zn2+-induced inhibition of glutamate uptake. Astrocytes were treated for 30 min with Zn2+ alone or with (A) 1 mM benzamide (BZ) or (B) 25 µM DPQ. (C) Comparison of Zn2+ effects on glutamate uptake in wild-type and PARP-1 deficient (PARP-1−/−) astrocytes. Glutamate uptake was assessed one hour after washout of Zn2+. Data points are means of three to four independent experiments (n = 3-4), each with measurements from two to three culture wells. *P< 0.05 compared with vehicle (A, B) or control (C) at the designated zinc concentration.

Zinc-Induced Glutamate Uptake Inhibition is Not Reversed by Subsequent Addition of a Zinc Chelator

Prior studies have shown that Zn2+ can inhibit glutamate uptake into the cells by a direct effect on glutamate transporters (30,40). This is an unlikely explanation for the present observations because astrocyte glutamate uptake capacity continued to fall long after washout of zinc; however, it is possible that Zn2+ could remain bound to cell membranes long after Zn2+ washout from the medium. To evaluate this possibility, an additional study was performed in which astrocytes were incubated with 1 mM of CaEDTA (a zinc chelator) (41) or 1 mM of ZnEDTA (control) for 5 min at three hours after Zn2+ exposure. These concentrations are in substantial excess of the original Zn2+ added to the culture wells. The inhibition of astrocyte glutamate uptake by Zn2+ was not reversed by incubation with the zinc chelator CaEDTA (Figure 3), thus arguing against an effect of retained zinc bound at the cell membranes.
Figure 3

The addition of a zinc chelator, CaEDTA, did not reverse the effect of zinc of glutamate uptake. Astrocytes were exposed for 30 min to Zn2+ at the designated concentrations, and glutamate uptake was measured three hours later. The cultures were also treated with 1 mM of the zinc chelator CaEDTA or, as a control, ZnEDTA, for 5 min prior to initiation of the glutamate uptake assay. Data points are means of three independent experiments (n = 3), each with measurements from two to three culture wells. *P < 0.05 compared with zero (0) zinc-exposed control.

Zn2+ Reduces Both Astrocyte ATP Levels and ATP/ADP Ratios

We proposed that zinc reduced glutamate uptake as a result of PARP-1 activation and resultant energy failure. To further test this idea, we measured the effect of Zn2+ on astrocyte ATP concentrations and ATP/ADP ratios. The basal ATP concentration was 20.3 ± 0.8 nmol/mg protein and the basal ATP/ADP ratio was 3.1. The ATP concentrations were decreased after Zn2+ (100–400 (µM) exposure in a time-dependent manner at both concentrations (Figure 4). The ATP/ADP ratio was also decreased by Zn2+, indicating an impairment in high-energy phosphorylation. The reductions in ATP concentrations and ATP/ADP ratios were both attenuated in astrocytes derived from PARP-1−/− mice (Figure 4).
Figure 4

Zn2+ affects astrocyte energy status in a PARP-1-dependent manner. (A) Astrocytes were exposed for 30 min to Zn2+ at the designated concentrations, and the levels of ATP and ADP were assessed immediately (zero hours), one hour, or three hours after zinc removal. Data points are means of three independent experiments (n = 3), each with measurements from two to three culture wells. *P< 0.05 versus controls. (B) Wild-type and PARP-1-deficient (PARP-1−/−) astrocytes were exposed for 30 min to Zn2+ at the designated concentrations and the levels of ATP and ADP were assessed immediately (zero hours), one hour, or three hours after zinc removal. Data points are means of four independent experiments (n = 4), each with measurements from two culture wells. *P< 0.05 versus wild-type astrocyte. (C) Zinc-induced changes in ATP / ADP ratio were also blocked in the PARP-1−/− cells. Data points are means of three independent experiments (n = 3), each with measurements from two culture wells. *P< 0.05 versus wild-type astrocyte.

Zinc-induced inhibition of glutamate uptake is not due to membrane disruption

These results support the idea that zinc-induced PARP-1 activation causes energy failure, which in turn leads to impaired glutamate uptake. However, an alternative possibility is that zinc-induced PARP-1 activation causes disruption of the cell membrane, and this is the proximate cause of ATP depletion and glutamate uptake failure. To evaluate this possibility we measured LDH activity retained the in the cultures at serial time points after zinc exposure. As shown in Figure 5, LDH activity in the intracellular compartment did not decrease until time points long after ATP depletion and glutamate uptake failure had occurred.
Figure 5

Zn2+ did not acutely cause cell membrane disruption. Astrocyte membrane integrity was evaluated by measuring the lactate dehydrogenase (LDH) retained in the cultures at serial time points after 30 min incubation with Zn2+. Data points are means of four independent experiments (n = 4), each with measurements from two culture wells. *P < 0.05 versus immediately (zero hours) after zinc removal.

Discussion

Zn2+ contributes to neuronal death in several conditions, including stroke, epilepsy, head trauma, and hypoglycemia, and intracerebroventricular administration of the zinc chelator CaEDTA reduces neuronal death (20, 21, 22, 23, 24, 25, 26, 27). It is generally assumed that zinc-induced neurotoxicity in these settings results from direct effects of zinc on the neurons. The present studies suggest an additional or alternative mechanism: zinc released from neurons may induce failure of astrocyte glutamate uptake through a mechanism involving PARP-1 activation and energy failure. The resulting increase in extracellular glutamate levels would be expected to contribute to neuronal demise, and activation of neuronal AMPA/kainate receptors could in turn stimulate additional Zn2+ release (18).

Astrocytes express both EAAT1 and EAAT2 glutamate transporter subtypes, with EAAT2 being responsible for the vast majority of glutamate uptake in most brain structures (8). Zn2+ has been previously reported to modulate glutamate uptake through direct effects on EAAT1 but not EAAT2 (30,42). Several lines of evidence argue that the inhibitory effect of Zn2+ on glutamate uptake observed in the present studies cannot be attributed to a direct effect of Zn2+ on glutamate transporters. First, the effect of Zn2+ incubations was delayed in onset and reached maximal effect 3 hours after washout of Zn2+ from the culture medium. Moreover, the uptake inhibition was not reversed by the addition of the very high affinity Zn2+ chelator, CaEDTA thereby excluding an effect mediated by residual Zn2+ bound to glutamate transporters or other cell membrane components. By contrast, the effect of Zn2+ on glutamate uptake was markedly attenuated both by pharmacological PARP inhibitors and by PARP-1 gene deletion.

The roughly parallel time course of glutamate uptake failure (see Figure 1) and ATP depletion (see Figure 4) further suggest a causative role for PARP-1 activation in the zinc-induced glutamate uptake failure. ATP-dependent processes are sensitive both to absolute ATP concentrations and the ATP/ADP ratio. Here, both of these measures declined after Zn2+ exposure, and these declines were blocked by PARP-1 gene deficiency. Consumption of cytosolic NAD+ by PARP-1 leads to a fall in the ATP/ADP ratio by impairing glycolysis and, indirectly, by impairing respiration (37,43,44) In addition, de novo synthesis of NAD+ is stimulated by NAD+ consumption and leads to depletion of the total ATP and adenylate pools (45). Thus reductions in both the ATP/ADP ratio and total ATP levels occur with extensive PARP-1 activation, and both may contribute to impaired glutamate uptake.

An unresolved question is which events may link the increased intracellular Zn2+ levels to increased PARP-1 activity. Possible candidate mediators are reactive oxygen species (ROS) such as superoxide ion, nitric oxide (NO), and peroxynitrite. In fact, several studies have previously reported that Zn2+ overload results in elevated intracellular levels of ROS in a PKC- and NADPH oxidase-dependent manner (16,46), suggesting that ROS generation may contribute to Zn2+-induced PARP-1 activation. NO, produced by NO synthases (NOS), is a well-established mediator of neuronal cell death in a variety of models of neuronal injury (47) in which Zn2+-induced cell death plays a prominent role (20,21,23,25).

Zn2+, released by neurons into the synapse and surrounding extracellular space during ischemia and other insults, may result in free Zn2+ concentrations of up to 100–400 µM in some brain regions (30, 31, 32). These concentrations are comparable to the levels of Zn2+ observed in the present studies to inhibit glutamate uptake. It should be noted, however, that there are several uncertainties regarding the extrapolation of these cell culture findings to the in vivo setting. First, protein binding of Zn2+ in vivo may lower true free Zn2+ activity (48). Second, a recent study using fluorescent indicators of free Zn2+ showed the extracellular levels achieved during ischemia to be much lower than the estimated maximal values (33). Third, it is possible that Zn2+ could have direct effects on neurons at concentrations well below those that cause impaired astrocyte glutamate uptake. On the other hand, Zn2+ released from intracellular protein binding sites may also contribute to Zn2+-mediated cell injury (49,50). Given these considerations, the present results indicate a potential mechanism by which neuronal Zn2+ release could lead to impaired astrocyte function and further neuronal injury, but additional studies will be required to confirm this process in vivo.

Notes

Acknowledgments

This work was supported by the Department of Veterans Affairs and by the National Institutes of Health grant RO1 NS41421 (R.A.S.). We thank Elizabeth Gum, Jennifer Bergher, and Jillian Silva for expert technical assistance.

References

  1. 1.
    Chen Y, Swanson RA. (2003) Astrocytes and brain injury. J. Cereb. Blood Flow Metab. 23:137–49.CrossRefGoogle Scholar
  2. 2.
    Swanson RA, Ying W, Kauppinen TM. (2004) astrocyte influences on ischemic neuronal death. Curr. Mol. Med. 4:193–205.CrossRefGoogle Scholar
  3. 3.
    Choi DW. (1988) Glutamate neurotoxicity and diseases of the nervous system. Neuron 1:623–34.CrossRefGoogle Scholar
  4. 4.
    Obrenovitch TP. (1995) The ischaemic penumbra: twenty years on. Cerebrovasc. Brain Metab. Rev. 7:297–323.PubMedGoogle Scholar
  5. 5.
    Wahl F, Obrenovitch TP, Hardy AM, Plotkine M, Boulu R, Symon L. (1994) Extracellular glutamate during focal cerebral ischaemia in rats: time course and calcium dependency. J. Neurochem. 63:1003–11.CrossRefGoogle Scholar
  6. 6.
    Rao VL, Bowen KK, Dempsey RJ. (2001) Transient focal cerebral ischemia down-regulates glutamate transporters GLT-1 and EAAC1 expression in rat brain. Neurochem. Res. 26:497–502.CrossRefGoogle Scholar
  7. 7.
    Anderson CM, Swanson RA. (2000) Astrocyte glutamate transport: review of properties, regulation, and physiological functions. Glia 32:1–14.CrossRefGoogle Scholar
  8. 8.
    Danbolt NC. (2001) Glutamate uptake. Prog. Neurobiol. 65:1–105.CrossRefGoogle Scholar
  9. 9.
    D’Amours D, Desnoyers S, D’Silva I, Poirier GG. (1999) Poly(ADP-ribosyl)ation reactions in the regulation of nuclear functions. Biochem. J. 342:249–68.CrossRefGoogle Scholar
  10. 10.
    Pieper AA, Verma A, Zhang J, Snyder SH. (1999) Poly (ADP-ribose) polymerase, nitric oxide and cell death. Trends Pharmacol. Sci. 20:171–81.CrossRefGoogle Scholar
  11. 11.
    Burzio LO, Riquelme PT, Koide SS. (1979) ADP ribosylation of rat liver nucleosomal core histones. J. Biol. Chem. 254:3029–37.PubMedGoogle Scholar
  12. 12.
    Zahradka P, Ebisuzaki K. (1982) Ashuttle mechanism for DNA-protein interactions. The regulation of poly(ADP-ribose) polymerase. Eur. J. Biochem. 127:579–85.CrossRefGoogle Scholar
  13. 13.
    Gaal JC, Pearson CK. (1985) Eukaryotic nuclear ADP-ribosylation reactions. Biochem. J 230:1–18.CrossRefGoogle Scholar
  14. 14.
    Berger NA. (1985) Poly(ADP-ribose) in the cellular response to DNA damage. Rad. Res. 101:4–15.CrossRefGoogle Scholar
  15. 15.
    Sheline CT, Behrens MM, Choi DW. (2000) Zinc-induced cortical neuronal death: contribution of energy failure attributable to loss of NAD(+) and inhibition of glycolysis. J. Neurosci. 20:3139–46.CrossRefGoogle Scholar
  16. 16.
    Kim YH, Koh JY. (2002) The role of NADPH oxidase and neuronal nitric oxide synthase in zinc-induced poly(ADP-ribose) polymerase activation and cell death in cortical culture. Exp. Neurol. 177:407–18.CrossRefGoogle Scholar
  17. 17.
    Sensi SL, Yin HZ, Carriedo SG, Rao SS, Weiss JH. (1999) Preferential Zn2+ influx through Ca2+-permeable AMPA/kainate channels triggers prolonged mitochondrial superoxide production. Proc. Natl. Acad. Sci. U. S. A. 96:2414–9.CrossRefGoogle Scholar
  18. 18.
    Weiss JH, Sensi SL, Koh JY. (2000) Zn(2+): a novel ionic mediator of neural injury in brain disease. Trends Pharmacol. Sci. 21:395–401.CrossRefGoogle Scholar
  19. 19.
    Sheline CT, Wang H, Cai AL, Dawson VL, Choi DW. (2003) Involvement of poly ADP ribosyl polymerase-1 in acute but not chronic zinc toxicity. Eur. J. Neurosci. 18:1402–9.CrossRefGoogle Scholar
  20. 20.
    Tonder N, Johansen FF, Frederickson CJ, Zimmer J, Diemer NH. (1990) Possible role of zinc in the selective degeneration of dentate hilar neurons after cerebral ischemia in the adult rat. Neurosci. Lett. 109:247–52.CrossRefGoogle Scholar
  21. 21.
    Koh JY, Suh SW, Gwag BJ, He YY, Hsu CY, Choi DW. (1996) The role of zinc in selective neuronal death after transient global cerebral ischemia. Science 272:1013–6.CrossRefGoogle Scholar
  22. 22.
    Calderone A, Jover T, Mashiko T, et al. (2004) Late calcium EDTA rescues hippocampal CA1 neurons from global ischemia-induced death. J. Neurosci. 24:9903–13.CrossRefGoogle Scholar
  23. 23.
    Frederickson CJ, Hernandez MD, McGinty JF. (1989) Translocation of zinc may contribute to seizure-induced death of neurons. Brain Res. 480:317–21.CrossRefGoogle Scholar
  24. 24.
    Suh SW, Thompson RB, Frederickson CJ. (2001) Loss of vesicular zinc and appearance of perikaryal zinc after seizures induced by pilocarpine. Neuroreport 12:1523–5.CrossRefGoogle Scholar
  25. 25.
    Suh SW, Chen JW, Motamedi M, et al. (2000) Evidence that synaptically-released zinc contributes to neuronal injury after traumatic brain injury. Brain Res. 852:268–73.CrossRefGoogle Scholar
  26. 26.
    Suh SW, Garnier P, Aoyama K, Chen Y, Swanson RA. (2004) Zinc release contributes to hypoglycemia-induced neuronal death. Neurobiol. Dis. 16:538–45.CrossRefGoogle Scholar
  27. 27.
    Suh SW, Frederickson CJ, Danscher G. (2006) Neurotoxic zinc translocation into hippocampal neurons is inhibited by hypothermia and is aggravated by hyperthermia after traumatic brain injury in rats. J. Cereb. Blood Flow Metab. 26:161–9.CrossRefGoogle Scholar
  28. 28.
    Howell GA, Welch MG, Frederickson CJ. (1984) Stimulation-induced uptake and release of zinc in hippocampal slices. Nature 308:736–8.CrossRefGoogle Scholar
  29. 29.
    Assaf SY, Chung SH. (1984) Release of endogenous Zn2+ from brain tissue during activity. Nature 308:734–6.CrossRefGoogle Scholar
  30. 30.
    Spiridon M, Kamm D, Billups B, Mobbs P, Attwell D. (1998) Modulation by zinc of the glutamate transporters in glial cells and cones isolated from the tiger salamander retina. J. Physiol. (Lond.) 506:363–76.CrossRefGoogle Scholar
  31. 31.
    Frederickson CJ, Koh JY, Bush AI. (2005) The neurobiology of zinc in health and disease. Nat. Rev. Neurosci. 6:449–62.CrossRefGoogle Scholar
  32. 32.
    Yokoyama M, Koh J, Choi DW. (1986) Brief exposure to zinc is toxic to cortical neurons. Neurosci. Lett. 71:351–5.CrossRefGoogle Scholar
  33. 33.
    Frederickson CJ, Giblin LJ, Krezel A, et al. (2006) Concentrations of extracellular free zinc (pZn)e in the central nervous system during simple anesthetization, ischemia and reperfusion. Exp. Neurol. 198:285–93.CrossRefGoogle Scholar
  34. 34.
    Swanson RA. (1992) Astrocyte glutamate uptake during chemical hypoxia in vitro. Neurosci. Lett. 147:143–6.CrossRefGoogle Scholar
  35. 35.
    Ying W, Swanson RA. (2000) The poly(ADP-ribose) glycohydrolase inhibitor gallotannin blocks oxidative astrocyte death. Neuroreport 11:1385–8.CrossRefGoogle Scholar
  36. 36.
    Wang ZQ, Stingl L, Morrison C, et al. (1997) PARP is important for genomic stability but dispensable in apoptosis. Genes Dev. 11:2347–58.CrossRefGoogle Scholar
  37. 37.
    Alano CC, Ying W, Swanson RA. (2004) Poly(ADP-ribose) polymerase-1-mediated cell death in astrocytes requires NAD+ depletion and mitochondrial permeability transition. J. Biol. Chem. 279:18895–902.CrossRefGoogle Scholar
  38. 38.
    Swanson RA, Farrell K, Simon RP. (1995) Acidosis causes failure of astrocyte glutamate uptake during hypoxia. J. Cereb. Blood Flow Metab. 15:417–24.CrossRefGoogle Scholar
  39. 39.
    Koh JY, Choi DW. (1987) Quantitative determination of glutamate mediated cortical neuronal injury in cell culture by lactate dehydrogenase efflux assay. J. Neurosci. Methods 20:83–90.CrossRefGoogle Scholar
  40. 40.
    Gabrielsson B, Robson T, Norris D, Chung SH. (1986) Effects of divalent metal ions on the uptake of glutamate and GABA from synaptosomal fractions. Brain Res. 384:218–23.CrossRefGoogle Scholar
  41. 41.
    Frederickson CJ, Suh SW, Koh JY, et al. (2002) Depletion of intracellular zinc from neurons by use of an extracellular chelator in vivo and in vitro. J. Histochem. Cytochem. 50:1659–62.CrossRefGoogle Scholar
  42. 42.
    Vandenberg RJ, Mitrovic AD, Johnston GA. (1998) Molecular basis for differential inhibition of glutamate transporter subtypes by zinc ions. Mol. Pharmacol. 54:189–96.CrossRefGoogle Scholar
  43. 43.
    Ying W, Alano CC, Garnier P, Swanson RA. (2005) NAD+ as a metabolic link between DNA damage and cell death. J. Neurosci. Res. 79:216–23.CrossRefGoogle Scholar
  44. 44.
    Zong WX, Ditsworth D, Bauer DE, Wang ZQ, Thompson CB. (2004) Alkylating DNAdamage stimulates a regulated form of necrotic cell death. Genes Dev. 18:1272–82.CrossRefGoogle Scholar
  45. 45.
    Zhang J, Dawson VL, Dawson TM, Snyder SH. (1994) Nitric oxide activation of poly(ADP-ribose) synthetase in neurotoxicity. Science 263:687–9.CrossRefGoogle Scholar
  46. 46.
    Noh KM, Koh JY. (2000) Induction and activation by zinc of NADPH oxidase in cultured cortical neurons and astrocytes. J. Neurosci. 20:RC111.CrossRefGoogle Scholar
  47. 47.
    Dawson VL. (1995) Nitric oxide: role in neurotoxicity. Clin. Exp. Pharmacol. Physiol. 22:305–8.CrossRefGoogle Scholar
  48. 48.
    Swanson RA, Sharp FR. (1992) Zinc toxicity and induction of the 72 kD heat shock protein in primary astrocyte culture. Glia 6:198–205.CrossRefGoogle Scholar
  49. 49.
    Lee JY, Cole TB, Palmiter RD, Koh JY. (2000) Accumulation of zinc in degenerating hippocampal neurons of ZnT3-null mice after seizures: evidence against synaptic vesicle origin. J. Neurosci. 20:RC79.CrossRefGoogle Scholar
  50. 50.
    Aizenman E, Stout AK, Hartnett KA, Dineley KE, McLaughlin B, Reynolds IJ. (2000) Induction of neuronal apoptosis by thiol oxidation: putative role of intracellular zinc release. J. Neurochem. 75:1878–88.CrossRefGoogle Scholar

Copyright information

© Feinstein Institute for Medical Research 2007

Authors and Affiliations

  • Sang Won Suh
    • 1
    • 2
  • Koji Aoyama
    • 1
    • 2
  • Conrad C. Alano
    • 1
    • 2
  • Christopher M. Anderson
    • 1
    • 2
  • Aaron M. Hamby
    • 1
    • 2
  • Raymond A. Swanson
    • 1
    • 2
  1. 1.Department of Neurology (127)University of CaliforniaSan FranciscoUSA
  2. 2.Department of Neurology (127)Veterans Affairs Medical CenterSan FranciscoUSA

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