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Local Impermeant Anions Establish the Neuronal Chloride Concentration

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Science  07 Feb 2014:
Vol. 343, Issue 6171, pp. 670-675
DOI: 10.1126/science.1245423

Causing Chloride Changes

Because intracellular chloride concentrations largely determine the direction and magnitude of current flow through GABAA channels, the stability of intracellular chloride concentration is important to maintain consistent synaptic inhibition. Glykys et al. (p. 670) examined the mechanisms by which chloride gradients in neurons are established, using chloride imaging with transgenically expressed clomeleon dye. Surprisingly, intracellular chloride was not primarily determined by transporters. Instead, subcellular gradients of immobile anions generated inverse chloride gradients.

Abstract

Neuronal intracellular chloride concentration [Cl]i is an important determinant of γ-aminobutyric acid type A (GABAA) receptor (GABAAR)–mediated inhibition and cytoplasmic volume regulation. Equilibrative cation-chloride cotransporters (CCCs) move Cl across the membrane, but accumulating evidence suggests factors other than the bulk concentrations of transported ions determine [Cl]i. Measurement of [Cl]i in murine brain slice preparations expressing the transgenic fluorophore Clomeleon demonstrated that cytoplasmic impermeant anions ([A]i) and polyanionic extracellular matrix glycoproteins ([A]o) constrain the local [Cl]. CCC inhibition had modest effects on [Cl]i and neuronal volume, but substantial changes were produced by alterations of the balance between [A]i and [A]o. Therefore, CCCs are important elements of Cl homeostasis, but local impermeant anions determine the homeostatic set point for [Cl], and hence, neuronal volume and the polarity of local GABAAR signaling.

The γ-aminobutyric acid type A (GABAA) receptor (GABAAR) can subserve either inhibition or excitation, because the net flux of the permeating anions HCO3 and Cl can be reversed by modest changes in the transmembrane concentration gradient of Cl (1, 2). NKCC1 and KCC2 are the primary cation-chloride cotransporters (CCCs) in neurons (3). Their unique stoichiometries result in distinct [Cl]i equilibria: ~3 mM for KCC2 (4, 5) and ~60 mM for NKCC1 (3). The species of cotransporter expressed in the neuron is thought to determine [Cl]i, but there is evidence that transporter expression is not the sole determinant of [Cl]i and, hence, the reversal potential for GABA (EGABA). First, CCCs transport water along with cations and Cl as nearly isotonic saline (6, 7). Neurons express no known aquaporin water channels (8), so the CCCs have limited capacity to alter [Cl]i independently of neuronal volume. Second, the transporter expressed may not correlate with the measured [Cl]i (9). Third, electrophysiological and fluorometric studies demonstrate a wide distribution of [Cl]i that rarely matches the equilibrium for either NKCC1 or KCC2 (1015). Finally, subcellular differences in EGABA indicate that [Cl]i is likely to vary within the cytoplasm of individual neurons (16, 17), a condition that cannot be efficiently maintained solely by transporters because of the high rate of dissipation of local [Cl]i by cytoplasmic diffusion (18).

A solution is suggested by the fact that Cl is only a minor component of the intracellular anionic milieu. The neuronal membrane is impermeable to most cytoplasmic anions, including phosphate groups associated with deoxy- and ribonucleotides, and the majority of intracellular proteins whose amino and carboxyl moieties are negatively charged at physiological pH (19). For any value of cytoplasmic volume and osmolarity, the sum of cytoplasmic impermeant anions ([A]i) and [Cl]i must be constant, as [HCO3] is fixed by pH requirements. Thus, [Cl]i should be constrained by [A]i. However, cotransport of Cl and cations across a membrane that is impermeant to [A]i creates an unstable Gibbs-Donnan condition with higher intracellular than extracellular osmotic pressure (20). The exclusion of Na+ from the cytoplasm by Na+- and K+-dependent adenosine triphosphatase (Na+,K+-ATPase) is thought to create a balancing Gibb-Donnan condition (7, 20), but this mechanism ignores intracellular K+ and is not supported by pharmacological inhibition of neuronal Na+,K+-ATPase (21). The sulfates on the proteoglycans of the extracellular matrix (22) make up a more plausible impermeant extracellular ion. Manipulation of extracellular proteoglycans alters cell volume, membrane potential, and neuronal network excitability, consistent with Donnan effects (23). We investigated whether [Cl]i is set by the local concentrations of impermeant anions on either side of the neuronal membrane.

Direct [Cl]i measurements were performed by using two-photon excitation microscopy imaging in acute and organotypic brain slices of mice expressing Clomeleon [ratiometric fluorophore sensitive to changes in [Cl]i (18)]. In neonatal neurons from CA1 hippocampal slices from postnatal day 8 to 9 (P8 to P9), where NKCC1 is the primary transporter expressed (24), there was a broad distribution of somatic [Cl]i of 14.7 ± 6.5 mM (median ± SD; n = 237 neurons; six slices) (Fig. 1, A and B). In adult CA1 hippocampal slices (P32 to P44), where KCC2 is the primary transporter (3), the somatic [Cl]i was also widely distributed 13.7 ± 8.9 mM (n = 227 neurons; eight slices) (Fig. 1C). Similar results were found in acute brain slices from neocortex layers IV/V and CA1 organotypic hippocampal slices (figs. S1, A and C, and S2, A and B; and tables S1 and S2). Thus, most neurons have [Cl]i not congruent with the equilibrium conditions of either KCC2 or NKCC1.

Fig. 1 [Cl]i is not solely determined by transport activity.

(A) Two-photon microscopy image of Clomeleon yellow fluorescent protein (YFP) from acute hippocampal slice CA1 (left) and neocortex layer IV/V (right). (Bottom) Detailed image of neuron outlined on right above. (B) P8 to P9 hippocampal slice. (Left) Initial versus new steady-state [Cl]i after 30-min NKCC1 block followed by an additional 30-min block of KCC2. Lines, linear fit. (Right) Similar to left but KCC2 block was first, then KCC2 and NKCC1 blocks came after. (C) As (B) but in P32 to P44 CA1 neurons. (D) Transporter index histogram of all neonatal hippocampal neurons (calculated as in methods and fig. S5), 2.5 ± 5.9 (n = 237; median ± SD). Black circle indicates expected value for canonical cooperation of KCC2 and NKCC1. (E) Transporter index of all recorded neonatal CA1 neurons (2.5 ± 5.9) and adult CA1 neurons (1.07 ± 5.6; n = 227) and expected values (neonatal: 16.7 ± 6.5; n = 237; adult: 15.7 ± 8.9; n = 227). *P < 0.001, Mann-Whitney rank-sum test. (F) (Top) [Cl]i from P6 to P8 layer IV/V neocortical pyramidal cells [soma (S): 16.0 ± 8.9 mM; axon (A): 13.9 ± 8.6 mM; dendrite (D): 11.5 ± 8.3 mM; difference among all three groups, P < 0.001, Friedman test; *P < 0.05 multiple-comparison Dunn’s method]. (Bottom) [Cl]i from P28 to P30 layer IV/V neocortical pyramidal cells [soma (S): 9.3 ± 6.1 mM; axon (A): 16.1 ± 7.9 mM; dendrite (D): 11.4 ± 6.5 mM; *P < 0.001]. (G) Subcellular gradient differences between axon-soma and dendrite-soma. Blockade of NKCC1 in neonates (10 μM bumetanide) and NKCC1 and KCC2 in adults (100 μM bumetanide) did not alter the subcellular [Cl]i gradients (paired neuron-process; P > 0.05; paired t test, error bars, SD).

If [Cl]i was primarily maintained by CCCs, the change in [Cl]i after transport block should be the opposite of the canonical direction of the primary expressed transporter: KCC2 block should increase [Cl]i; NKCC1 block should decrease [Cl]i. In neonatal CA1 slices (P8 to P9), blocking NKCC1 with bumetanide 10 μM did not alter [Cl]i (15.8 ± 7.6 to 16 ± 7.3 mM, n = 105 paired cells) (Fig. 1B and fig. S3A). Addition of 10 μmol of the specific KCC2 antagonist VU0240551 (25) induced a minimal decrease in [Cl]i to 15 ± 6.9 mM (Fig. 1B and fig. S3A), and [Cl]i did not become passively distributed across the membrane such that the reverse potential for Cl (ECl) ≈ resting membrane potential. After CCC block, [Cl]i increased in neurons with a low initial [Cl]i and decreased in neurons with a high initial [Cl]i (fig. S3A), regardless of the order of antagonist application (Fig. 1B and fig. S3B) in adult CA1 slices (P32 to P44) (Fig. 1C and fig. S3, C and D), in CA1 organotypic hippocampal slices after 6 to 11 days in vitro (DIV6 to DIV11) (fig. S2, A to C and E to G), and in acute layer IV/V neocortical pyramidal neurons (P8 to P9 and P27 to P31) (fig. S1 and tables S1 and S2). If no drug was added, [Cl]i was stable (fig. S4, C to E). In summary, the initial [Cl]i was a better predictor of the change in [Cl]i than was the species of blocked transporter. To quantify this, we summed the absolute values of the change in [Cl]i during sequential block of KCC2 and NKCC1. If NKCC1 and KCC2 are working against each other in the same neuron to create a broad distribution of [Cl]i, this sum value should be large (fig. S5). However, this sum was nearly 0 in all neuronal populations studied (Fig. 1, D and E, and fig. S2, D and H). Therefore, the broad distribution of [Cl]i cannot be explained by the net effects of oppositely directed NKCC1 and KCC2 cotransport.

[Cl]i varies not only between neurons but also between subcellular regions (16), which is difficult to reconcile with the high intracellular mobility of [Cl]i (18). We measured millimolar differences in [Cl]i at the soma versus the proximal 40 μm of the axon and the proximal 200 μm of the apical dendrites of neonatal and adult neocortical neurons (sparse neocortical expression of Clomeleon permitted identification of individual processes and soma) (Fig. 1F). Subcellular differences in [Cl]i were not maintained by local CCCs because, after CCC block, [Cl]i gradients were unchanged (P > 0.05, paired t test) (Fig. 1G).

These data are not consistent with the hypothesis that [Cl]i is determined by the species of expressed cotransporter. Rather, the data suggest that KCC2 and NKCC1 both serve as conduits for transmembrane Cl flux whose direction is determined by other factor(s). We therefore tested the hypothesis that [A]i and the polyanionic extracellular matrix glycoproteins [A]o determine the local [Cl] and, thus, ECl and the effect of GABAA receptor activation.

Prediction 1. If the sum of [A]i + [Cl]i is constant, then the broad distribution of [Cl]i, together with the large intercellular variance in the primary constituents of [A]i [cytoplasmic protein and nucleic acid concentrations (26)], can be used to test for the predicted reciprocal relation between [A]i and [Cl]i. [A]i and [Cl]i were imaged in Clomeleon organotypic hippocampal slice cultures to facilitate the prolonged dye incubation required to estimate [A]i. CA1 pyramidal neurons demonstrated a wide range of somatic [Cl]i of 14.8 ± 6.3 mM at DIV10 to DIV12 (n = 305 neurons; four slices) (Fig. 2, A to C). After Cl imaging, slices were incubated for 2 hours in SYTO64 10 μM, which binds to the cytoplasmic-nuclear nucleic acids whose phosphate groups are a major component of [A]i. SYTO64 staining intensity was negatively correlated with [Cl]i [correlation coefficient (R) = –0.3; P < 0.001] (Fig. 2, B and C). Because nucleic acids make up approximately one-third of intracellular fixed anions (27), the strength of the correlation between SYTO64 staining and [Cl]i is what would be predicted if [A]i sets [Cl]i.

Fig. 2 Correlation of [A]i and [A]o with neuronal [Cl]i.

(A) (Left) Two-photon microscopy z-stack image of YFP (green) from CA1 pyramidal layer in an organotypic hippocampal slice from a Clomeleon-expressing mouse. (Middle) SYTO64 staining (red) of cytoplasmic and nuclear nucleic acids overlaid on the YFP image. (Boxes) YFP and SYTO64 fluorescence in individual neurons. (Right) Pseudo-colored neurons on the basis of the YFP/CFP (cyan fluorescent protein) ratio. (B) [Cl]i as a function of SYTO64 staining. R = –0.29, P = 0.01; n = 70 neurons; one slice. (C) [Cl]i as a function of normalized SYTO64 staining. R = –0.3, P < 0.001; n = 305 neurons; four slices. Line, linear fit. (D to F) Correlation between sulfated extracellular matrix and [Cl]i. (D) Confocal images of Alcian blue staining in CA1 pyramidal layer of an organotypic hippocampal slice. Outlined area magnified on right. (E) [Cl]i distribution before Alcian blue staining. Outlines: Region of interest used to calculate average [Cl]i and Alcian blue staining intensity. (F) Alcian blue staining of slice in (E), transmitted light. (G) Correlation between [Cl]i and extracellular matrix (Alcian blue staining) obtained in each region of interest, four slices. Error bars, SD; AU, arbitrary units. Line, linear fit (P < 0.001).

Prediction 2. If the sum of [A]i and [Cl]i is constant, then increasing [A]i should decrease [Cl]i. [A]i was increased by iso-osmotic perfusion of 20 mM gluconate, pyruvate, and d-lactate, which are weak organic acids that are transported across the cytoplasmic membrane (28). Each perfusion reduced [Cl]i by 5 to 10%, consistent with a corresponding increase in [A]i due to a Nernstian distribution of the deprotonated, anionic bases at a resting membrane potential near –70 mV (fig. S6). This was unlikely a pH effect on Clomeleon fluorescence, because the pHi effects (29) would alter Clomeleon fluorescence in the opposite direction from those observed (18). Thus, increases in [A]i are accompanied by reductions in [Cl]i, so that the sum of [A]i + [Cl]i is constant.

Prediction 3. If [A]o sets the local extracellular chloride concentration [Cl]o, then cation-chloride cotransport should come to equilibrium at a [Cl]i that reflects the local [Cl]o.. Thus, [A]o should vary inversely with [Cl]i. The polysulfated proteoglycans of the extracellular matrix create extracellular negative charge densities of 50 to 350 mEq/liter and, thus, could compose [A]o (30). We first verified that extracellular Na+ does not exert a significant Donnan effect (21) (fig. S7). Next, [Cl]i was measured in organotypic Clomeleon hippocampal slices (DIV12 to DIV14). Then, slices were fixed and incubated with Alcian blue at pH 0.5 to specifically stain sulfated glycosaminoglycans (31). [A]o as assayed by Alcian blue staining was negatively correlated with [Cl]i (R = –0.7, P < 0.001) (Fig. 2, D to G, and fig. S8). These data support the possibility that polysulfated proteoglycans of the extracellular matrix make up [A]o and that, together with [A]i, these macromolecular anions constrain the local [Cl] to set the local ECl.

Prediction 4. Decreasing [A]o will increase [Cl]i..If the sulfated carbohydrate moieties of the proteoglycans in the extracellular matrix subserve this function, then their lysis would release SO4 and reduce [A]o. This would increase local [Cl]o and shift the equilibrium condition for transmembrane cation-chloride transport toward higher [Cl]i. Accordingly, when organotypic hippocampal slices (DIV12 to DIV14) were incubated in chondroitinase ABC (ChABC) for 1 hour, neuronal [Cl]i increased from 5.9 ± 3.4 to 20.2 ± 5.7 mM (n = 47 neurons; four slices, P < 0.0001, Wilcoxon signed rank test) (Fig. 3, A to E). The [Cl]i change was significantly higher (P < 0.0001) than that by incubation with vehicle solution (from 9.2 ± 2.7 to 10.9 ± 4.3 mM, n = 43; four slices, P = 0.02). Somatic volume was unchanged at ~80 min (Fig. 3, B, D, and E), which likely reflects successful compensatory volume regulation. Cell viability was not altered by incubation in ChABC (fig. S9).

Fig. 3 [Cl]i is changed by disruption of the extracellular matrix and by increased extracellular osmolarity.

(A) Pseudo-colored, two-photon microscopy z-stack image before and after incubation with chondroitinase ABC (ChABC) in an organotypic hippocampal slice. (B) Significant effect of ChABC on [Cl]i, but not volume. (C) [Cl]i change by incubation with vehicle versus ChABC solution (vehicle: +0.8 ± 3.9 mM, n = 43; four slices; ChABC: +15.8 ± 3.8 mM, n = 47; four slices; P < 0.0001, unpaired t test). (D) As in (C) but plotting somatic volume (vehicle; –52 ± 174 μm3, ChABC; –23 ± 203 μm3, P = 0.46 unpaired t test. Change in vehicle: 1699 ± 480 to 1647 ± 464 μm3, P = 0.08. Change in ChABC: 1905 ± 564 to 1882 ± 516 μm3, P = 0.51, Wilcoxon signed rank test, same cells as (C). (E) Volume versus [Cl]i changes for each neuron in (C) and (D). *P < 0.0001. (F and G) Organotypic hippocampal slices expressing Clomeleon (two-photon microscopy) after increasing osmolarity with 20 mM mannitol (8% increase) and in bumetanide (G). (H and I) [Cl]i and neuronal volume changes in mannitol (H) and mannitol plus bumetanide (I). (J and K) [Cl]i and neuronal somatic volume changes induced by increased extracellular osmolarity. (L) Neuronal volume changes as a function of [Cl]i changes.

Prediction 5. In a system in which [A]i, [A]o, and [Cl]i are in ionic and osmotic equilibrium, acutely altering the osmotic balance should alter [Cl]i. Water is transported with cations and Cl by CCCs (6, 7), and neurons lack known aquaporins (8). Thus, water movement contributes to the free energy of cotransport (6). An increase in extracellular osmolarity would favor CCC movement of water and Cl out of the neuron, increasing the fractional cytoplasmic concentration of [A]i and decreasing [Cl]i. This is opposite to what would be predicted by free transmembrane water permeability: Loss of intracellular water would increase [Cl]i (7). Two-photon multiplanar micrographs of individual pyramidal cells from organotypic hippocampal slices (DIV8 to DIV12) expressing Clomeleon were reconstructed in three dimensions to measure volume and [Cl]i (Fig. 3, F to I). In control conditions, the somatic volume and [Cl]i were stable as a function of time (fig. S4). Increasing extracellular osmolarity by 8% [from 261 (the osmolarity of culture medium) to 281 mOsm] via the addition of 20 mM mannitol resulted in a rapid 21% decrease in somatic volume from 2333 ± 1192 to 1842 ± 967 μm3 (mean ± SD, n = 73 neurons; four slices; P < 0.001, paired t test) and a 9% decrease in somatic [Cl]i from 16.6 ± 14.6 to 15.1 ± 11.1 mM (P < 0.001, Wilcoxon signed rank test) (Fig. 3, H, J, and L). Using the same protocol but blocking NKCC1 and KCC2 (with bumetanide 200 μM) resulted in a 9% decrease in somatic volume from 2365 ± 1005 to 2147 ± 953 μm3 (n = 68 neurons; three slices; P < 0.0001, paired t test) (Fig. 3, I and K) and no change in somatic [Cl]i from 7.1 ± 10 to 8.3 ± 7.9 mM (P = 0.074, Wilcoxon signed rank test) (Fig. 3, I to L). The unlinking of volume and [Cl]i changes when CCCs were blocked is likely to represent volume regulation by other systems (7).

Finally, a consequence of the cotransport of water and salt by NKCC1 and KCC2 is that near-isotonic saline moves across the membrane, so that both neuronal volume and [Cl]i should change in parallel during cotransport. Several conditions—including hypoxic ischemic injury, trauma, and prolonged seizures—have in common the development of cytotoxic edema and increased neuronal [Cl]i (15, 32, 33). To test whether seizure-induced increases in neuronal volume are associated with acute increases in [Cl]i, we performed extracellular field recording and two-photon microscopy to measure cytoplasmic volume and [Cl]i in organotypic hippocampal slice cultures (DIV10 to DIV12) that spontaneously develop ictal-like epileptiform discharges (34). Prolonged seizure activity increased both neuronal volume and [Cl]i (Fig. 4). Somatic volume increased by 10% from 2530 ± 1658 to 2775 ± 1741 μm3 (mean ± SD; n = 42 neurons; four slices; P = 0.006, paired t test) and [Cl]i increased from 25.4 ± 7.4 to 40.8 ± 13.8 mM (P < 0.001, Wilcoxon signed rank test). The increase in [Cl]i during seizures is mediated by NKCC1 as it can be reduced by bumetanide (15).

Fig. 4 [Cl]i and intracellular volume changes during ictal activity.

(A) [Cl]i transients during spontaneous seizures in the CA1 pyramidal cell layer, organotypic hippocampal slice (DIV12). (Top) Pseudo-colored, two-photon images of CA1 neurons before and during seizures. (Middle) Extracellular field-potential recording. (Bottom) [Cl]i changes in a population of neurons (median, black; SD, red lines; green dotted line indicates initial [Cl]i). (B) Extracellular recording of spontaneous seizure in CA1 region of organotypic hippocampal slice (DIV12). (Bottom) Two-photon microscopy z-stack image of neurons before and during spontaneous seizure. (C) [Cl]i and somatic volume changes in individual neurons during spontaneous seizure activity (*P < 0.05). (D to F) [Cl]i and somatic volume changes during recurrent seizures (n = 40 neurons; four slices).

These data indicate that the local [A]i and [A]o determine [Cl]i,, [Cl]o, and, therefore, EGABA, and CCCs serve to maintain [Cl]i at this set point. Therefore, (i) the widely observed intercellular and intracellular variances in [Cl]i and EGABA are best explained by local variation in [A]i and [A]o. The species of CCC and other cellular features are likely to correlate with [A]i and [Cl]i [e.g., (14, 24)]. (ii) The developmental reduction in [Cl]i would follow from the increase in neuronal [A]i during development (35) and experience (36), paralleled by increases in the proteoglycans of the extracellular matrix (37). (iii) The subcellular variance in [Cl]i arises from corresponding differences in the concentrations of relatively immobile cytoplasmic macromolecular anions (38). The variance in [A]i creates intracytoplasmic Gibbs-Donnan effects (39), such that local [Cl]i is at equilibrium at different local [A]i. Thus, CCCs are not required to compensate for intracytoplasmic Cl diffusion. (iv) The influence of [A]o and [A]i on local [Cl]i, and [Cl]o open possibilities for developmental and experience-dependent plasticity of EGABA and Eglycine at individual synapses, so that the variance in extracellular sulfated proteoglycans composes a potential locus of analog information storage and pathologically, a rich variety of antigens. (v) Pathological conditions that alter [A]o or [A]i will have secondary effects on both cell volume and [Cl]i. This may explain the correlation between magnetic resonance imaging evidence of cytotoxic edema after brain injury and anticonvulsant-resistant seizures, which can occur when increased [Cl]i compromises GABAAR-mediated inhibition (15, 40). Thus, the magnitude and direction of GABAAR currents at individual synapses are among the wide variety of signaling functions subserved by intra- and extracellular macromolecular networks.

Supplementary Materials

www.sciencemag.org/content/343/6171/670/suppl/DC1

Materials and Methods

Figs. S1 to S10

Tables S1 and S2

References

References and Notes

  1. Acknowledgments: This work was supported by National Institute of Neurological Disorders and Stroke, NIH, grant NS 40109-06 the Kennedy Endowment for Child Neurology and Mental Retardation. J.G. was supported by the American Epilepsy Society postdoctoral fellowship and NIH R25. K.E. was supported by The Japan Foundation for Pediatric Research. K.T.K. was supported by the Manton Center for Orphan Disease Research and NIH R25.
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