Differential maturation of chloride homeostasis
Differential maturation of chloride homeostasis
Differential maturation of chloride homeostasis
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Int. J. Devl Neuroscience 25 (2007) 479–489<br />
www.elsevier.com/locate/ijdevneu<br />
<strong>Differential</strong> <strong>maturation</strong> <strong>of</strong> <strong>chloride</strong> <strong>homeostasis</strong> in primary<br />
afferent neurons <strong>of</strong> the somatosensory system<br />
Daniel Gilbert a,1 , Christina Franjic-Würtz a , Katharina Funk a ,<br />
Thomas Gensch b , Stephan Frings a, *, Frank Möhrlen a<br />
a Department <strong>of</strong> Molecular Physiology, University <strong>of</strong> Heidelberg, Im Neuenheimer Feld 230, 69120 Heidelberg, Germany<br />
b Institute for Neuroscience and Biophysics 1, Juelich Research Center, Leo-Brand-Strasse, 52425 Juelich, Germany<br />
Received 16 June 2007; received in revised form 23 July 2007; accepted 6 August 2007<br />
Abstract<br />
Recent research into the generation <strong>of</strong> hyperalgesia has revealed that both the excitability <strong>of</strong> peripheral nociceptors and the transmission <strong>of</strong> their<br />
afferent signals in the spinal cord are subject to modulation by Cl currents. The underlying Cl <strong>homeostasis</strong> <strong>of</strong> nociceptive neurons, in particular<br />
its postnatal <strong>maturation</strong>, is, however, poorly understood. Here we measure the intracellular Cl concentration, [Cl ] i , <strong>of</strong> somatosensory neurons in<br />
intact dorsal root ganglia <strong>of</strong> mice. Using two-photon fluorescence-lifetime imaging microscopy, we determined [Cl ] i in newborn and adult<br />
animals. We found that the somatosensory neurons undergo a transition <strong>of</strong> Cl <strong>homeostasis</strong> during the first three postnatal weeks that leads to a<br />
decline <strong>of</strong> [Cl ] i in most neurons. Immunohistochemistry showed that a major fraction <strong>of</strong> neurons in the dorsal root ganglia express the cation–<br />
<strong>chloride</strong> co-transporters NKCC1 and KCC2, indicating that the molecular equipment for Cl accumulation and extrusion is present. RT-PCR<br />
analysis showed that the transcription pattern <strong>of</strong> electroneutral Cl co-transporters does not change during the <strong>maturation</strong> process.<br />
These findings demonstrate that dorsal root ganglion neurons undergo a developmental transition <strong>of</strong> <strong>chloride</strong> <strong>homeostasis</strong> during the first three<br />
postnatal weeks. This process parallels the developmental ‘‘<strong>chloride</strong> switch’’ in the central nervous system. However, while most CNS neurons<br />
achieve homogeneously low [Cl ] i levels – which is the basis <strong>of</strong> GABAergic and glycinergic inhibition – somatosensory neurons maintain a<br />
heterogeneous pattern <strong>of</strong> [Cl ] i values. This suggests that Cl currents are excitatory in some somatosensory neurons, but inhibitory in others. Our<br />
results are consistent with the hypothesis that Cl <strong>homeostasis</strong> in somatosensory neurons is regulated through posttranslational modification <strong>of</strong><br />
cation–<strong>chloride</strong> co-transporters.<br />
# 2007 ISDN. Published by Elsevier Ltd. All rights reserved.<br />
Keywords: Pain; Nociceptors; Dorsal root ganglia; Chloride <strong>homeostasis</strong>; Chloride transporters; Fluorescence-lifetime imaging<br />
1. Introduction<br />
Neuronal activity can be strongly influenced by Cl currents.<br />
Inhibitory Cl currents mediate GABAergic and glycinergic<br />
inhibition in the CNS. Excitatory Cl currents occur in neurons<br />
which accumulate Cl , as described for immature neurons <strong>of</strong> the<br />
CNS (Ben-Ari, 2002), for olfactory sensory neurons (Kaneko<br />
Abbreviations: 2P-FLIM, two-photon fluorescence-lifetime imaging<br />
microscopy; [Cl ] i , intracellular <strong>chloride</strong> concentration; CGRP, calcitoningene<br />
related peptide; MQAE, N-6-methoxyquinolinium acetoethylester;<br />
TRPV1, transient receptor potential vanilloid receptor type 1.<br />
* Corresponding author. Tel.: +49 6221 54 5661; fax: +49 6221 54 5627.<br />
E-mail address: s.frings@zoo.uni-heidelberg.de (S. Frings).<br />
1 Current address: Department <strong>of</strong> Physiology and Pharmacology, University<br />
<strong>of</strong> Queensland, Brisbane, QLD 4072, Australia.<br />
et al., 2004), for neurons in spinal and autonomic ganglia (review,<br />
Frings et al., 2000), as well as for neurons challenged by<br />
ischemia, inflammation, or neurological disorders (Payne et al.,<br />
2003; Pond et al., 2006; De Koninck, 2007). The balance<br />
between inhibitory and excitatory Cl effects is determined by<br />
Cl uptake and Cl extrusion pathways active in each<br />
cell. Studies <strong>of</strong> neuronal Cl <strong>homeostasis</strong> have indicated that<br />
the Na + –K + –2Cl co-transporter NKCC1 provides the main<br />
route for Cl uptake, while KCC2 couples Cl extrusion to K +<br />
efflux. It is generally held that NKCC1 expression dominates in<br />
immature neurons <strong>of</strong> cortex and hippocampus, and that KCC2<br />
expression is only induced after birth (Lu et al., 1999; Rivera<br />
et al., 1999; Stein et al., 2004). This developmental transition –<br />
<strong>of</strong>ten termed ‘‘<strong>chloride</strong> switch’’ – shifts the Cl -equilibrium<br />
potential, E Cl , from values near 40 mV to values near the<br />
resting voltage. Once this transition is completed (in rats and<br />
0736-5748/$30.00 # 2007 ISDN. Published by Elsevier Ltd. All rights reserved.<br />
doi:10.1016/j.ijdevneu.2007.08.001
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D. Gilbert et al. / Int. J. Devl Neuroscience 25 (2007) 479–489<br />
mice 2 weeks after birth), the opening <strong>of</strong> Cl channels stabilizes<br />
the resting voltage.<br />
In contrast to CNS neurons, primary afferent neurons <strong>of</strong> the<br />
peripheral nervous system (e.g. somatosensory neurons and<br />
olfactory sensory neurons) are believed to mature without<br />
undergoing a transition <strong>of</strong> <strong>chloride</strong> <strong>homeostasis</strong>, and to support<br />
depolarizing Cl currents throughout the adult life. In olfactory<br />
sensory neurons, E Cl is maintained near 0 mV in adult animals,<br />
and a depolarizing Cl efflux carries the main part <strong>of</strong> the odorinduced<br />
receptor current (Reuter et al., 1998; Kaneko et al.,<br />
2004). A similar role is assumed for Cl currents in<br />
somatosensory neurons, based on reports <strong>of</strong> elevated Cl<br />
levels (30–50 mM) in dorsal root ganglion neurons (Gallagher<br />
et al., 1978; Alvarez-Leefmans et al., 1988; Kenyon, 2001;<br />
Kaneko et al., 2002). Furthermore, somatosensory neurons can<br />
respond to GABA with depolarization (Rudomin and Schmidt,<br />
1999; Sung et al., 2000). Finally, the expression <strong>of</strong> NKCC1<br />
(Alvarez-Leefmans et al., 2001; Kanaka et al., 2001), combined<br />
with the hardly detectable levels <strong>of</strong> KCC2 mRNA (Rivera et al.,<br />
1999; Kanaka et al., 2001), is interpreted as indicative <strong>of</strong> Cl<br />
accumulation. However, two observations are not easily<br />
reconciled with the general concept <strong>of</strong> excitatory Cl currents<br />
in somatosensory neurons: (1) the measured E Cl values (around<br />
40 mV) limit the excitatory effect <strong>of</strong> Cl currents and may<br />
even oppose strong depolarization and excitation; (2) NKCC1<br />
mRNA was detected in only 50% <strong>of</strong> somatosensory neurons in<br />
dorsal root ganglia and trigeminal ganglia, where it is colocalized<br />
with TRPV1 (Price et al., 2006). This expression<br />
pattern may indicate that excitatory Cl currents are restricted<br />
to certain modalities <strong>of</strong> the somatosensory system.<br />
To approach the question <strong>of</strong> Cl accumulation and its role in<br />
the somatosensory system, we examined the <strong>maturation</strong> <strong>of</strong> Cl<br />
<strong>homeostasis</strong> after birth. We directly measured [Cl ] i in intact<br />
dorsal root ganglion neurons <strong>of</strong> early postnatal and adult mice<br />
using two-photon fluorescence-lifetime imaging microscopy<br />
(2P-FLIM). We looked at the expression <strong>of</strong> NKCC1 and KCC2<br />
protein in rat dorsal root ganglia. To assess possible<br />
contributions <strong>of</strong> other Cl transporters to the <strong>maturation</strong> <strong>of</strong><br />
Cl <strong>homeostasis</strong>, we examined the transcription pattern <strong>of</strong> all<br />
genes that encode electroneutral cation–<strong>chloride</strong> co-transporters<br />
in newborn and adult rats.<br />
2. Experimental procedures<br />
2.1. Isolation <strong>of</strong> somatosensory neurons for calibration<br />
All experimental procedures were performed in accordance with the Animal<br />
Protection Law and the guidelines and permissions <strong>of</strong> Heidelberg University.<br />
Adult female NMRI (Naval Medical Research Institute, USA) mice were<br />
anesthetized and killed by cervical transsection. The spinal column was<br />
prepared and opened sagittally with scissors. Thirty to forty dorsal root ganglia<br />
were dissected from the lumbar, thoracic and cervical region. Ganglia were cut<br />
into small pieces and incubated in 2 ml <strong>of</strong> collagenase solution (0.3% collagenase,<br />
C-9891, Sigma, Germany, in DMEM) for 1 h at 37 8C. After<br />
centrifugation (200 g, 20 min) the supernatant was discarded, and 2 ml <strong>of</strong><br />
trypsin solution (0.25% trypsin, T-1426, Sigma, in MEM) was added to the<br />
pellet. The pellet was resuspended by trituration with a truncated, fire-polished<br />
Pasteur pipette (3 mm opening). The ganglia were kept in trypsin solution for<br />
30 min at 37 8C, and then centrifuged for 20 min at 200 g. The supernatant<br />
was discarded and 4 ml <strong>of</strong> culture medium (DMEM + 10% FCS, 10106-169,<br />
and 1% antibiotics/antimycotics, 15240-062, Gibco Life Technologies, Invitrogen,<br />
Karlsruhe, Germany) was added to the pellet. The pellet was triturated, and<br />
then filtered through a 150 mm nylon mesh (Typ 1110, Bückmann, Germany).<br />
This step removes a substantial amount <strong>of</strong> myelin debris and non-dissociated<br />
fragments <strong>of</strong> ganglia, which are retained on the nylon mesh. The pooled cells<br />
were plated on coverslips (coated with 100 mg/ml poly-L-lysine, P-1399,<br />
Sigma, and 20 mg/ml laminin, L-2020, Sigma) and cultured at 37 8C in culture<br />
medium under an atmosphere containing 5% CO 2 . Nerve growth factor (NGF-b<br />
from rat, N-2513, Sigma) was added 1 h after plating at a final concentration <strong>of</strong><br />
50 ng/ml. Cultures were used within 24 h after plating. Cells were incubated in<br />
standard extracellular solution (Table 1) containing 5 mM MQAE (N-6-methoxyquinolinium<br />
acetoethylester; Molecular Probes, Invitrogen) for at least<br />
30 min in the dark, at 37 8C. The dye progressively accumulates within the<br />
cells as the molecule is rendered membrane impermeable by cytosolic esterases<br />
(Koncz and Daugirdas, 1994) with only minor effects on its fluorescence<br />
properties (Kaneko et al., 2002). After incubation, extracellular MQAE was<br />
washed away and coverslips were transferred to the FLIM instrument.<br />
2.2. Tissue preparations for 2P-FLIM measurements<br />
Newborn or adult female NMRI mice were anesthetized and killed by<br />
cervical transsection. The backbone was prepared and vertebrae containing the<br />
spinal cord with attached dorsal root ganglia were isolated with a razor blade<br />
from the spinal column. All preparations were done in cooled (4 8C) standard<br />
extracellular solution (Table 1). Only those vertebrae were used for 2P-FLIM<br />
measurements whose dorsal root ganglia had an intact dura mater and which<br />
were connected to undamaged dorsal roots and spinal nerves. Preparations were<br />
incubated in standard extracellular solution containing 5 mM MQAE for 3.5 h<br />
at room temperature (20 8C). After incubation, the dye solution was replaced by<br />
standard extracellular solution and the preparations were stored at 4 8C until the<br />
measurement. For 2P-FLIM recordings, MQAE-loaded preparations were<br />
immobilized with low melting agarose (USB Corporation, USA) at the bottom<br />
<strong>of</strong> 6 cm dishes (Greiner, Germany). All recordings were done at room temperature<br />
in standard extracellular solution. To test the viability <strong>of</strong> neurons in the<br />
preparation during the time <strong>of</strong> the 2P-FLIM experiments, we performed<br />
viability tests with 0.5 mg/ml MTT (3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium<br />
bromide; Molecular Probes), and with 0.4% trypan blue (Gibco<br />
Life Technologies). Following the preparation, the tissues were incubated at<br />
room temperature in standard extracellular solution and were subsequently<br />
loaded with either MTT (60 min) or trypan blue (10 min) at various times.<br />
Using this method, we established a time window <strong>of</strong> 5 h post mortem during<br />
which the viability <strong>of</strong> DRG neurons was good and the tissue could be used for<br />
2P-FLIM analysis.<br />
2.3. Two-photon fluorescence-lifetime imaging microscopy (2P-<br />
FLIM)<br />
MQAE was used as a fluorescent probe for intracellular Cl ([Cl ] i )<br />
(Verkman, 1990). MQAE molecules reach the excited state upon absorption<br />
<strong>of</strong> a single ultraviolet photon (l = 375 nm) or, alternatively, the simultaneous<br />
absorption <strong>of</strong> two infrared photons (l = 750 nm). We used two-photon excita-<br />
Table 1<br />
Solutions (in mM)<br />
Na K Ca Mg Cl NO 3<br />
Standard extracellular solution 140 5 2.5 1 151<br />
15 Cl standard solution 150 15 105<br />
30 Cl standard solution 150 30 120<br />
45 Cl standard solution 150 45 105<br />
60 Cl standard solution 150 60 90<br />
75 Cl standard solution 150 75 75<br />
Solutions contained 10 mM glucose; pH 7.4 was buffered with 10 mM HEPES.<br />
The cell isolation solution was buffered with phosphate (in mM: 1.9 NaH 2 PO 4 ,<br />
8.1 Na 2 HPO 4 ).
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tion to achieve an optical resolution <strong>of</strong> 0.5 mm(x-/y-plane) and 1 mm(z-axis).<br />
The infrared light used for two-photon excitation caused no detectable photodamage,<br />
even with the relatively long observation times <strong>of</strong> multiple images with<br />
1 min <strong>of</strong> illumination per image. For the MQAE molecule, the dwell time in the<br />
excited singlet state (the fluorescence lifetime, t) is near 30 ns in water<br />
containing 50 mM MQAE and is reduced by anions through collisional quenching.<br />
The Cl dependence <strong>of</strong> t is described by the Stern–Volmer relation<br />
(t 0 /t =1+K SV [Cl ] i ), where t 0 is the fluorescence lifetime in 0 mM Cl<br />
and K SV , the Stern–Volmer constant, is a measure <strong>of</strong> the Cl sensitivity <strong>of</strong><br />
MQAE. K SV has a value <strong>of</strong> 185 M 1 in water but only 3–20 M 1 inside cells<br />
(Lau et al., 1994; Bevensee et al., 1997; Maglova et al., 1998; Eberhardson et al.,<br />
2000; Kaneko et al., 2002). This reduced sensitivity <strong>of</strong> intracellular MQAE may<br />
result in part from interactions <strong>of</strong> the dye with other soluble anions and from<br />
self-quenching <strong>of</strong> MQAE at concentrations >100 mM(Kaneko et al., 2002). For<br />
2P-FLIM measurements, the tissues or cells were placed on the stage <strong>of</strong> an<br />
upright fluorescence microscope (BX50WI; Olympus Optical, Japan) and<br />
observed through a 60 water-immersion objective (n.a. = 0.9; Olympus<br />
Optical). Fluorescence was excited with 150 fs light pulses (l = 750 nm)<br />
applied at sufficient intensity to generate two-photon excitation. Light pulses<br />
were generated at a frequency <strong>of</strong> 75 MHz by a mode-locked Titan-Sapphire<br />
laser (Mira 900; output power >500 mW; Coherent, Santa Clara, USA), which<br />
was pumped by the frequency-doubled output (532 nm) <strong>of</strong> a Nd–vanadate laser<br />
(Verdi; Coherent). The laser light was directed through the objective to the<br />
tissue surface at reduced power (2.5 mW) using a beam scanner (TILL<br />
Photonics, Munich, Germany). Fluorescence was recorded by photomultipliers,<br />
and lifetime analysis was performed using electronics (SPC-730; Becker &<br />
Hickl, Berlin, Germany) and s<strong>of</strong>tware (SPC7.22; Becker & Hickl) for timecorrelated<br />
single-photon counting (Lakowicz, 1999). Lifetime images were<br />
analyzed using SPCImage 1.8 and 2.6 (Becker & Hickl) and a self-made image<br />
analysis s<strong>of</strong>tware. A detailed description <strong>of</strong> the instrument and the calibration<br />
procedure is described in Kaneko et al. (2002). Images were obtained by<br />
scanning the excitation light focus through tissue layers 1–3 cells below the<br />
dura mater. Mean values <strong>of</strong> Cl concentrations are given with standard<br />
deviations (S.D.).<br />
2.4. Single cell-based quantitative analysis <strong>of</strong> 2P-FLIM data<br />
For quantification <strong>of</strong> cytosolic fluorescence lifetimes, we developed a<br />
s<strong>of</strong>tware that enables single cell-based analysis in 2P-FLIM z-scan images.<br />
The cytosolic MQAE signal <strong>of</strong> a single neuron was analyzed at the equatorial<br />
layer, i.e. the optical section in the image stack, where the total area <strong>of</strong> the cell<br />
was largest. The cytosolic region was outlined by defining manually two regions<br />
<strong>of</strong> interest, delimiting the margins <strong>of</strong> the nucleus and <strong>of</strong> the cell, respectively.<br />
The quantitative parameters, mean fluorescence lifetime (in ns) and cell<br />
diameter (in mm), were extracted by the s<strong>of</strong>tware. The cell diameter, d, was<br />
calculated according to d = H(4A/p), with A = area <strong>of</strong> the cell, assuming<br />
circular cell morphology. The diameter is an important parameter, because<br />
sensory modalities <strong>of</strong> dorsal root ganglion neurons are <strong>of</strong>ten correlated with this<br />
value (e.g. Petruska et al., 2002).<br />
2.5. Immunohistochemistry<br />
To examine the expression <strong>of</strong> Cl transport proteins, we used rat instead <strong>of</strong><br />
mouse dorsal root ganglia because the available antibodies were better suited<br />
for rat than for mouse tissue. Four dorsal root ganglia were dissected from the<br />
thoracic spinal cord <strong>of</strong> two adult Wistar rats and immersed in 4% paraformaldehyde<br />
in PBS (8.1 mM Na 2 HPO 4 , 1.9 mM NaH 2 PO 4 , 130 mM NaCl, pH 7.4)<br />
for 25 min. After three washing steps in PBS, the tissue was sequentially<br />
dehydrated in 10–30% sucrose overnight. Tissue was then embedded in Tissue-<br />
Tek (Leica, Nussloch, Germany) and frozen onto the cryostate stage (Leica CM<br />
3050 S). Four to eight cryosections (12 mm) were cut and collected on coated<br />
slides (SuperFrost 1 Plus, Menzel, Braunschweig, Germany). Sections were airdried<br />
for 30 min, post-fixed in 4% paraformaldehyde in PBS, washed three<br />
times in PBS and blocked in 5% ChemiBLOCKER TM (Millipore, Billerica,<br />
USA), 0.5% Triton X100 in PBS. Primary antibodies were diluted in the same<br />
buffer and incubated for 2 h. The following antibodies and dilutions were used:<br />
mouse anti-NKCC1 1:20 (T4, monoclonal antibody, obtained from the Developmental<br />
Studies Hybridoma Bank, The University <strong>of</strong> Iowa), goat anti-NKCC1<br />
1:20 (N-16; Santa Cruz Biotech, Heidelberg, Germany, #sc-21545), goat anti-<br />
KCC2 1:20 (Santa Cruz Biotech, #sc-19420). After three washing steps in PBS,<br />
sections were incubated for 90 min in fluorescent-labeled donkey anti-mouse<br />
Alexa594 (Invitrogen, A-21203, 1:500) or donkey anti-goat Alexa488 (Invitrogen,<br />
A-21206, 1:500) secondary antibodies. After three washing steps in PBS, a<br />
0.3 mM DAPI solution (Fluka, #32670) was used to stain the nuclei. Sections<br />
were coverslipped with Aqua Poly/Mount (Polysciences, Warrington, USA) and<br />
analyzed using a Nikon Eclipse 90i upright automated microscope equipped<br />
with a Nikon DS-1QM CCD camera. The instrument was used at the Nikon<br />
Imaging Center at the University <strong>of</strong> Heidelberg. No fluorescence signal was<br />
observed upon omission <strong>of</strong> primary antibodies. To test for the specificity <strong>of</strong><br />
primary antibodies, preadsorption controls were performed for the NKCC1 (N-<br />
16) and the KCC2 polyclonal antibodies using a fivefold excess <strong>of</strong> blocking<br />
peptides (0.05 mg/ml) according to the manufacturer’s specifications. No<br />
immunosignal was observed after preadsorption. The specificity <strong>of</strong> the monoclonal<br />
T4 antibody for NKCC1 was demonstrated by Chen et al. (2005) through<br />
the absence <strong>of</strong> T4 immunosignals in brain tissue <strong>of</strong> NKCC1 / mice. Two slices<br />
were evaluated for each test. To avoid double counting <strong>of</strong> cells, every fourth to<br />
sixth section was evaluated, ensuring a minimum distance <strong>of</strong> 24–48 mm<br />
between individual sections.<br />
2.6. Expression <strong>of</strong> electroneutral cation–<strong>chloride</strong> co-transporter<br />
genes<br />
Dorsal root ganglia and, for controls, kidney and brain were dissected from<br />
adult and newborn (P1) Wistar rats. Total RNA was extracted following the<br />
protocol <strong>of</strong> Chomczynski and Sacchi (1987). After DNase I treatment (RNasefree,<br />
Fermentas, StLeon-Rot, Germany) cDNA was synthesized from 5 mg total<br />
RNA using an oligo-dT primer and Superscript TM III Reverse Transcriptase<br />
(Invitrogen) according to the manufacturer’s instructions. The cDNA was<br />
quantified for normalization using PCR (16, 20, 24, 28 and 32 cycles) with<br />
b-actin and ATPase primers. The annealing temperature for all primers was<br />
58 8C. Semi-quantitative PCR amplification was performed on 0.5 ml singlestranded<br />
cDNA product with 2U Taq DNA polymerase (Fermentas). The<br />
cycling conditions were 94 8C for 3 min, 94 8C for 30 s, 58 8C for 30 s,<br />
72 8C for 1 min for 28 and 32 cycles, respectively, and 72 8C for 8 min. For<br />
each cation–<strong>chloride</strong> co-transporter gene, primer pairs were: CCC9/F, 5 0 -TCA<br />
CTG TGT TTG GGG TGT TC-3 0 ; CCC9/R, 5 0 -GGA GAG GGC GAA GTA<br />
AGA GTA G-3 0 ; CCC6/F, 5 0 -GGT TCA ACG GAA GCA CCC TAA-3 0 ; CCC6/<br />
R, 5 0 -GTG ACC ACA GCA GCC AAT GT-3 0 ; KCC1/F, 5 0 -TGA CCC TAG<br />
TGG TGT TTG TCG G-3 0 ; KCC1/R, 5 0 -GTT CCT GCT GAC GCC ATC A-3 0 ;<br />
KCC2/F, 5 0 -GTC TCT GGG CCC GGA GTT T-3 0 ; KCC2/R, 5 0 -GGC ATC CCG<br />
CAG GTC TC-3 0 ; KCC3/F, 5 0 -TGC TGC TGT ACA ATG TTA ACT GCC-3 0 ;<br />
KCC3/R, 5 0 -TAG CCA ACC CTG GAATGC C-3 0 ; KCC4/F, 5 0 -TGC TTT CTA<br />
TCC TGG CCA TCT ATG-3 0 ; KCC4/R, 5 0 -GCC TCC CCA AAC TTA TCT<br />
CGC-3 0 ; NKCC1/F, 5 0 -CGA ATTATT GGA GCC ATTACA GT-3 0 ; NKCC1/R,<br />
5 0 -ACATCT GGA AAG CTG GGT AGATA-3 0 ; NKCC2/F, 5 0 -ATT CAATGA<br />
TGG TGG ATC CAA C-3 0 ; NKCC2/R, 5 0 -CGG CGATGA GAATGA ATG C-<br />
3 0 ; TSC/F, 5 0 -GTA GAC CCC ATC AAT GAC ATC C-3 0 ; TSC/R, 5 0 -AAG CCA<br />
ATC AGA GGG TAC AGC-3 0 . For positive controls and normalization b-actin<br />
and Na + /K + -ATPase primer pairs were: Actin/F, 5 0 -GGT CAT CAC TAT CGG<br />
CAA TGA GC-3 0 ; Actin/R, 5 0 -GGA CAG TGA GGC CAG GAT AGA GC-3 0 ;<br />
ATPase/F, 5 0 -AGT GAG CTG AAA CCC ACG TAC C-3 0 and ATPase/R, 5 0 -<br />
CCC CTC TTT GTA GCC GTA GGA TT-3 0 . The resulting PCR products were<br />
cloned into pGMT vector (Promega, Mannheim, Germany) and sequenced.<br />
3. Results<br />
In a previous study <strong>of</strong> olfactory sensory neurons, we<br />
observed that these neurons were incapable <strong>of</strong> maintaining<br />
elevated [Cl ] i after cell isolation (Kaneko et al., 2004). In the<br />
present study we, therefore, measured [Cl ] i without isolating<br />
the somatosensory neurons from their ganglia. Moreover, the<br />
protein expression pattern in isolated somatosensory neurons<br />
changes during dedifferentiation processes in culture (Scott and<br />
Edwards, 1980), and this may alter the control <strong>of</strong> [Cl ] i .To
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obtain information about [Cl ] i values in situ, we performed<br />
<strong>chloride</strong> imaging in dorsal root ganglia with intact dura mater<br />
and intact axonal connections with the spinal cord. Isolated<br />
neurons were only used for calibrating the 2P-FLIM signal, as<br />
the manipulation <strong>of</strong> [Cl ] i by ionophores was more efficient<br />
when the neurons were dissociated.<br />
3.1. Somatosensory neurons undergo a postnatal <strong>chloride</strong><br />
transition<br />
The neurons in MQAE-loaded dorsal root ganglia displayed<br />
different fluorescence intensities when illuminated with the<br />
excitation light (Fig. 1a, black-and-white image). The fluorescence<br />
intensity, however, does not report [Cl ] i because it is<br />
co-determined by the unknown dye concentration in each cell.<br />
Fluorescence originating from the nuclei was weak. This may<br />
be caused by poor dye loading <strong>of</strong> the nuclei or by different<br />
quenching conditions in the nucleoplasm. The nuclear signals<br />
where excluded from further analyses. The fluorescence<br />
lifetime, t, which is proportional to [Cl ] i and can be used<br />
as intracellular Cl reporter (Koncz and Daugirdas, 1994;<br />
Kaneko et al., 2002), was colour-coded and is displayed as 2P-<br />
FLIM image for the same cells (Fig. 1a, colour image). In the<br />
2P-FLIM images, warmer colours indicate higher levels <strong>of</strong><br />
[Cl ] i . To establish the quantitative relation between 2P-FLIM<br />
signals and [Cl ] i in MQAE-loaded dorsal root ganglion<br />
neurons, we set [Cl ] i in isolated neurons to 1–5 levels (15, 30,<br />
45, 60, 75 mM) using a double ionophore technique. Isolated<br />
neurons in primary culture were used because the manipulation<br />
<strong>of</strong> [Cl ] i was more efficient in single cells than in intact ganglia.<br />
The neurons were kept in a solution containing the required<br />
Cl concentration (Table 1) as well as 40 mM tributyltin (a Cl /<br />
OH exchanger) and 20 mM nigericin (a K + /H + exchanger).<br />
The combination <strong>of</strong> these ionophores has been shown to<br />
dissipate Cl gradients across the plasma membrane (Chao<br />
et al., 1989). Fluorescence lifetimes decreased from 3.7 to<br />
3.1 ns when [Cl ] i was raised from 15 to 75 mM within the<br />
cytosol (15 mM: 3.73 0.17 ns, n = 16; 30 mM: 3.66 <br />
0.09 ns, n = 4; 45 mM: 3.45 0.14 ns, n =5; 60mM:<br />
3.43 0.07 ns, n = 13; 75 mM: 3.14 0.13 ns, n = 10). A<br />
Stern–Volmer plot <strong>of</strong> the calibration data (Fig. 1b) yielded a<br />
quenching constant <strong>of</strong> 3.05 M 1 , which was used in all further<br />
experiments to calculate [Cl ] i from the measured lifetimes.<br />
We have previously tested the reliability <strong>of</strong> this calibration<br />
procedure in primary afferent neurons <strong>of</strong> the olfactory system.<br />
In a comparison <strong>of</strong> 2P-FLIM analysis (Kaneko et al., 2004) and<br />
<strong>chloride</strong> measurements by energy-dispersive X-ray microanalysis<br />
(Reuter et al., 1998), the measured [Cl ] i values differed<br />
Fig. 1. Determination <strong>of</strong> [Cl ] i in somatosensory neurons by 2P-FLIM. (a) Comparison <strong>of</strong> fluorescence intensity (left) and lifetime (right) images from the same<br />
dorsal root ganglion. The intensity image shows strong signals from the cytosol and weak signals from the nuclei. In the 2P-FLIM image, the fluorescence lifetime, t,<br />
is colour-coded with warmer colours representing higher [Cl ] i levels. (b) Calibration <strong>of</strong> 2P-FLIM signals in isolated dorsal root ganglion neurons with [Cl ] i set to<br />
the indicated values using the two-ionophore method. The solid line represents a least-squares fit to the data using the Stern–Volmer equation t 0 /t =1+K SV [Cl ] i<br />
with K SV = 3.05 M 1 . The colour scale illustrates the false-colour representation <strong>of</strong> [Cl ] i in the following 2P-FLIM images. (c) 2P-FLIM images illustrating [Cl ] i<br />
levels in somatosensory neurons from newborn (P1–P4) and adult (third week) mice. The calibration established in (b) was used for false-colour representation <strong>of</strong><br />
[Cl ] i . Newborn neurons show almost uniformly high [Cl ] i (70 mM). During <strong>maturation</strong>, most somatosensory neurons decrease their [Cl ] i to some extent,<br />
resulting in a heterogeneous mosaic <strong>of</strong> [Cl ] i levels in the ganglia <strong>of</strong> mature animals.
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by less than 20%. For this reason, we give all absolute Cl<br />
concentrations in the present study with a confidence range<br />
<strong>of</strong> 20%.<br />
We determined [Cl ] i in somatosensory neurons in intact<br />
ganglia by focusing the excitation light <strong>of</strong> the 2P-FLIM<br />
instrument through the dura mater into cells 20–100 mm deep<br />
inside the ganglion. Deeper cell layers were not accessible for<br />
analysis because the dye did not sufficiently load the cells at<br />
distances > 100 mm from the dura mater. To determine [Cl ] i<br />
in neurons <strong>of</strong> newborn mice, preparations <strong>of</strong> 1–4 days old<br />
animals (P1–P4) were examined by 2P-FLIM. Since the<br />
<strong>chloride</strong> transition develops between P6 and P14 (Rivera et al.,<br />
2005), we expected to find in the P1–P4 animals the high levels<br />
<strong>of</strong> [Cl ] i characteristic for embryonal and early postnatal<br />
neurons. Indeed, the somatosensory neurons exhibited uniformly<br />
high levels <strong>of</strong> [Cl ] i (Fig. 1c, P1–P4). Single cell-based<br />
quantitative analysis <strong>of</strong> 975 neurons (pooled from P1 to P4)<br />
yielded a distribution <strong>of</strong> [Cl ] i between 35 and 120 mM with a<br />
mean [Cl ] i <strong>of</strong> 77.2 mM (S.D. = 13.6 mM) (Fig. 2).<br />
2P-FLIM measurements in the third postnatal week revealed a<br />
decrease <strong>of</strong> [Cl ] i in most cells, and a heterogeneous distribution<br />
<strong>of</strong> [Cl ] i levels among different neurons, ranging from 10 to<br />
>80 mM [Cl ] i (Fig. 1c). The general decline <strong>of</strong> [Cl ] i indicates<br />
a pr<strong>of</strong>ound change in <strong>chloride</strong> <strong>homeostasis</strong> with reduced Cl<br />
uptake and/or enhanced Cl extrusion. In adult animals (12–15<br />
weeks), the heterogeneous distribution was maintained (Fig. 1c).<br />
A histogram <strong>of</strong> [Cl ] i values obtained from 818 neurons in eight<br />
ganglia from six adult animals is shown in Fig. 2. The mean value<br />
is significantly lower than in P1–P4 animals (Student’s t-test:<br />
p 0.0005), and the distribution is broad (mean: 61.8 mM,<br />
S.D. = 19.7 mM). Both postanatal and adult data could be<br />
Fig. 2. Distribution <strong>of</strong> [Cl ] i values in dorsal root ganglia <strong>of</strong> newborn and adult<br />
mice. The histograms show the distribution <strong>of</strong> measured [Cl ] i levels in<br />
newborn (closed circles) and adult (open circles) animals. During the course<br />
<strong>of</strong> <strong>maturation</strong>, the distribution <strong>of</strong> [Cl ] i shifts towards lower levels. The lines<br />
compare global fits to the data with a single Gaussian distribution (dashed lines)<br />
and with three Gaussian distributions (solid lines). The three populations<br />
contributing to the latter fit are characterized by mean [Cl ] i levels <strong>of</strong><br />
37.8 mM, 58.7 mM, and 80.5 mM, and their relative contributions change<br />
during <strong>maturation</strong> from 0 to 18.9%, from 21 to 55.2%, and from 79 to<br />
25.9%, respectively.<br />
tentatively described by a sum <strong>of</strong> three Gaussian distributions<br />
with mean values <strong>of</strong> 37.8 mM, 58.7 mM and 80.5 mM [Cl ] i ,<br />
respectively (Fig. 2). During the developmental transition, the<br />
percentage <strong>of</strong> ‘‘high-<strong>chloride</strong> cells’’ decreased from 79 to 26%,<br />
that <strong>of</strong> ‘‘medium-<strong>chloride</strong> cells’’ increased from 21 to 55%, and<br />
that <strong>of</strong> ‘‘low-<strong>chloride</strong> cells’’ from 0 to 19%. Our data demonstrate<br />
that the somatosensory neurons in an individual ganglion <strong>of</strong> an<br />
adult animal exhibit a differential pattern <strong>of</strong> <strong>chloride</strong> <strong>homeostasis</strong>.<br />
Most neurons undergo a transition <strong>of</strong> the <strong>chloride</strong><br />
<strong>homeostasis</strong> during <strong>maturation</strong>, while roughly a third <strong>of</strong> the cells<br />
maintain the high [Cl ] i levels <strong>of</strong> the early postnatal days.<br />
3.2. Lack <strong>of</strong> correlation between [Cl ] i and cell size<br />
The size <strong>of</strong> somatosensory neurons can be indicative <strong>of</strong> their<br />
sensory modalities. Small and medium-sized somata (B-cells;<br />
mean volume: 10,700 mm 3 ; Tandrup, 2004) are <strong>of</strong>ten polymodal<br />
nociceptors or heat-sensitive cells with unmyelinated C-<br />
fibres. Large-diameter neurons (A-cells; mean volume:<br />
57,200 mm 3 ; Tandrup, 2004) mediate proprioception, touch<br />
or other low-threshold sensations. While detailed information<br />
about protein expression patterns, conduction velocities, and<br />
excitation properties is required to establish the specific<br />
modality <strong>of</strong> a somatosensory neuron (Guo et al., 1999; Lawson,<br />
2002; Fang et al., 2006), the cell size can serve as a first<br />
indication for the sensory system involved. To find out whether<br />
the different [Cl ] i levels in adult neurons correspond to any<br />
specific cell size, we measured the diameters <strong>of</strong> all neurons<br />
analyzed for Fig. 2, and related them to the measured [Cl ] i<br />
values. Since the 2P-FLIM images represent optical slices <strong>of</strong><br />
about 1 mm thickness, an individual image may show either the<br />
maximal (equatorial) diameter <strong>of</strong> a cell or, alternatively, a<br />
smaller (non-equatorial) diameter. For our analysis, we<br />
determined the maximal diameter for each individual cell.<br />
[Cl ] i was determined in the cytosolic region <strong>of</strong> each neuron,<br />
excluding the nucleus (Fig. 3a, arrows). The plot <strong>of</strong> [Cl ] i<br />
versus cell diameter does not reveal any correlation between the<br />
two parameters in adult neurons (Fig. 3b, black dots; linear<br />
regression analysis: r 2 = 0.019, n = 818). Both small-diameter<br />
cells (15–25 mm) and larger neurons cover the entire range <strong>of</strong><br />
measured [Cl ] i levels. The mean values (Fig. 3c) illustrate an<br />
increase <strong>of</strong> the mean cell diameter from 17.5 2.8 to<br />
25.8 6.3 mm and a decrease <strong>of</strong> mean [Cl ] i from<br />
77.2 13.6 to 61.8 19.7 mM during <strong>maturation</strong>. However,<br />
the <strong>chloride</strong> transition appears not to be restricted to a cell<br />
population with a distinct size. This finding suggests that a<br />
change in the regime <strong>of</strong> <strong>chloride</strong> handling occurs during<br />
postnatal <strong>maturation</strong> in somatosensory neurons <strong>of</strong> various<br />
sensory modalities.<br />
3.3. Expression <strong>of</strong> NKCC1 and KCC2 proteins<br />
A possible explanation for the mosaic pattern <strong>of</strong> [Cl ] i levels<br />
in adult dorsal root ganglia could be that some cells express<br />
predominantly NKCC1 while others express mainly KCC2. To<br />
test this hypothesis, we double-stained cryosections <strong>of</strong> dorsal<br />
root ganglia with antibodies raised against the two proteins. To
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Fig. 3. Heterogeneous [Cl ] i levels in mouse somatosensory neurons <strong>of</strong> various sizes. (a) 2P-FLIM images show the nuclear region in many cells with fluorescence<br />
signals distinct from the cytosol. To determine [Cl ] i , the fluorescence lifetime was evaluated in the cytosolic region, illustrated as the area between two circles<br />
(arrows). To determine the cell size, a series <strong>of</strong> images (z-stack) was analyzed, and the maximal diameter <strong>of</strong> each individual cell was measured. (b) Dot plot relating<br />
[Cl ] i to cell diameter for 975 neurons from early postnatal animals (red) and 818 neurons from adult animals (black). No correlation between cell size and [Cl ] i is<br />
detectable. (c) Mean [Cl ] i decreased from 77.2 13.6 to 61.8 19.7 mM, while the mean cell diameter increased from 17.5 2.8 to 25.8 6.3 mm during<br />
<strong>maturation</strong>.<br />
detect NKCC1 expression, we used two different antibodies:<br />
the monoclonal T4 antibody (raised against a C-terminal<br />
epitope <strong>of</strong> NKCC1; Lytle et al., 1995) which was demonstrated<br />
to be appropriate for somatosensory neurons (Alvarez-Leefmans<br />
et al., 2001), and the polyclonal N-16 antibody (raised<br />
against an N-terminal epitope <strong>of</strong> NKCC1, Santa Cruz). Of 534<br />
cells, 450 (84%) were stained with the T4 antibody. Co-staining<br />
with T4 and N-16 antibodies revealed a highly consistent<br />
pattern (Fig. 4a–c). Two hundred and forty-nine small- and<br />
medium-diameter neurons were examined. Eighty-one percent<br />
<strong>of</strong> these (202 cells) were positive for both antibodies, 5% (12<br />
cells) showed only a T4 signal, and 14% (35 cells) were not<br />
stained. Thus, 94% <strong>of</strong> T4-positive neurons were also N-16<br />
positive, which represents strong evidence for NKCC1<br />
expression in most somatosensory neurons. Immunosignals<br />
from the KCC2 antibody were significantly weaker than those<br />
from NKCC1. Seventy-six percent <strong>of</strong> 285 small-to-medium<br />
sized cells were immunopositive for KCC2, and 91% <strong>of</strong> these<br />
were also stained with the T4 antibody (Fig. 4d–f). In summary,<br />
expression <strong>of</strong> KCC2 appears to be distinctly weaker than that <strong>of</strong><br />
NKCC1. While most <strong>of</strong> the somatosensory neurons coexpressed<br />
NKCC1 and KCC2, a subpopulation <strong>of</strong> 20% <strong>of</strong><br />
the small-to-medium size neurons express NKCC1 without<br />
detectable KCC2 expression.<br />
3.4. Invariant transcription <strong>of</strong> electroneutral cation–<br />
<strong>chloride</strong> transporters during <strong>maturation</strong><br />
The change <strong>of</strong> [Cl ] i during postnatal development may be<br />
the consequence <strong>of</strong> altered expression <strong>of</strong> Cl transporters in the<br />
somatosensory neurons. To test whether an altered transcription<br />
program causes the Cl transition, we examined the mRNA
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Fig. 4. Expression <strong>of</strong> electroneutral cation–<strong>chloride</strong> co-transporters in rat somatosensory neurons. (a–c) Immunohistochemistry with two antibodies directed against<br />
NKCC1. The immunosignals <strong>of</strong> the antibodies T4 (C-terminal) and N-16 (N-terminal) match, with only few neurons missing the N-16 signal (red cells in c). (d–f)<br />
Expression <strong>of</strong> KCC2 is detectable but weak in most somatosensory neurons. No immunostain was observed after preadsorption <strong>of</strong> the polyclonal antibodies (N-16 and<br />
KCC2) with their respective immunization peptides (not shown). Nuclei are stained blue with DAPI.<br />
expression <strong>of</strong> all nine electroneutral cation–<strong>chloride</strong> cotransporters<br />
present in the rat genome (synonym: solute carrier<br />
family 12, SLC12; review, Gamba, 2005) by semi-quantitative<br />
RT-PCR. We made first-strand cDNA from dorsal root ganglia<br />
<strong>of</strong> newborn (P1) and adult animals. The relative concentrations<br />
<strong>of</strong> the cDNAs in the RT-PCR assays were adjusted using the<br />
highly abundant b-actin and the less abundant Na + /K + -ATPase<br />
as internal standards (Fig. 5a). The cDNAs were amplified with<br />
primers specific for CCC6, CCC9, KCC1-4, NKCC1-2 and<br />
TSC. CCC6 and CCC9 are orphan members <strong>of</strong> the SLC12<br />
family with unknown function, while TSC is the thiazidesensitive<br />
Na + –Cl co-transporter (for gene identification see<br />
legend to Fig. 5). Cycling conditions were adjusted to 28 and 32<br />
cycles. Fig. 5b demonstrates that the mRNA <strong>of</strong> five Cl cotransporters<br />
(CCC6, KCC1, KCC3, KCC4, NKCC1) could be<br />
detected by 28 PCR cycles from both P1 and adult animals.<br />
Fig. 5c indicates that 32 PCR cycles reached the amplification<br />
plateau for the five co-transporters listed above. In addition, a<br />
diagnostic signal <strong>of</strong> CCC9, KCC2 and TSC was observed,<br />
while no NKCC2 signal could be detected. Generating PCR<br />
amplification products under these conditions may be<br />
influenced by template abundance or by primer efficiency.<br />
To distinguish between these alternatives, we amplified KCC2<br />
from normalized brain cDNA, as well as NKCC2 and TSC from<br />
normalized kidney cDNA. Strong signals were detected by 32<br />
PCR cycles (Fig. 5a, right). Since no tissue-specific expression<br />
data were available for CCC9, the respective control was<br />
performed on adult dorsal root ganglia cDNA only and showed<br />
a strong signal with 36 cycles (Fig. 5a, right). These data<br />
indicate that each <strong>of</strong> the primer pairs used in this study<br />
exhibited similar efficiency. Therefore, the yield <strong>of</strong> the PCR<br />
amplification products depended only on the level <strong>of</strong> input<br />
template. All primer pairs were designed to span intron/exon<br />
boundaries, to reveal possible genomic DNA contamination.<br />
None <strong>of</strong> the PCR reactions showed amplification <strong>of</strong> genomic<br />
DNA which would have given rise to correspondingly larger<br />
DNA fragments. For unambiguous identification, all PCR<br />
products were eluted from agarose gels, cloned into the vector<br />
pGMT and sequenced.<br />
In summary, we found high expression levels <strong>of</strong> CCC6,<br />
KCC1, KCC3, KCC4 and NKCC1, much lower expression<br />
levels for CCC9, KCC2 and TSC, while no expression for<br />
NKCC2 mRNA was observed. Most importantly, the mRNA<br />
expression patterns <strong>of</strong> P1 and adult animals could not be<br />
distinguished on the grounds <strong>of</strong> the semi-quantitative PCR data.<br />
These results clearly demonstrate that the <strong>maturation</strong> <strong>of</strong> Cl<br />
<strong>homeostasis</strong> cannot be attributed to changes in the transcription<br />
pattern <strong>of</strong> electroneutral cation–<strong>chloride</strong> co-transporters.<br />
4. Discussion<br />
In trying to assess the role <strong>of</strong> Cl accumulation in<br />
somatosensory signal generation, we have examined the<br />
question whether Cl <strong>homeostasis</strong> changes after birth. We
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Fig. 5. Expression <strong>of</strong> electroneutral cation–<strong>chloride</strong> co-transporters in dorsal root ganglia (DRG) <strong>of</strong> newborn (P1) and adult rats. Semi-quantitative RT-PCR assays<br />
were used to determine expression levels <strong>of</strong> mRNA transcripts encoding cation–<strong>chloride</strong> co-transporter 9 (CCC9; synonym: solute carrier family 12 member 8,<br />
SLC12A8; GenBank accession NM_153625), cation–<strong>chloride</strong> co-transporter 6 (CCC6; synonyms: cation–<strong>chloride</strong> co-transporter-interacting protein, CIP;<br />
SLC12A9; NM_134405), K–Cl co-transporter 1 (KCC1, SLC12A4; NM_019229), K–Cl co-transporter 2 (KCC2; SLC12A5; NM_134363), K–Cl co-transporter<br />
3 (KCC3; SLC12A6; XM_001066756), K–Cl co-transporter 4 (KCC4; SLC12A7; XM_001060536), Na–K–Cl co-transporter 1 (NKCC1, SLC12A2; NM_031798),<br />
Na–K–Cl co-transporter 2 (NKCC2, SLC12A1; NM_019134), thiazide-sensitive Na–Cl co-transporter (TSC; SLC12A3; NM_019345). The primers were specific for<br />
the individual subtypes <strong>of</strong> co-transporters and were designed to span several exons to control for the possible presence <strong>of</strong> genomic DNA in the RNA preparation.<br />
Cycles <strong>of</strong> amplification are indicated for each reaction. The figures are negative images <strong>of</strong> ethidium bromide-stained agarose gels. DNA marker (M): 100 bp ladder.<br />
(a) The cDNA concentrations were normalized by amplification (16, 20, 24, 28 and 32 cycles) with b-actin and ATPase primers, and 0.5 ml <strong>of</strong> cDNA product was used<br />
per amplification. For positive controls, KCC2, NKCC2 and TSC were amplified from kidney or brain cDNA, and CCC9 was amplified with 36 cycles from dorsal<br />
root ganglia cDNA <strong>of</strong> adult animals. (b) Strong signals were observed for CCC6, KCC1, KCC3, KCC4 and NKCC1 in either P1 or adult animals using 26 cycles <strong>of</strong><br />
amplification. No expression was detected under these conditions for CCC9, KCC2, NKCC2 and TSC. (c) Amplification begins to plateau within 32 cycles for CCC6,<br />
KCC1, KCC3, KCC4 and NKCC1 in P1 and adult animals. Weak expression was detected for CCC9, KCC2 and TSC in cDNA from P1 and adult animals. No<br />
expression was detected for NKCC2.<br />
measured [Cl ] i in the somata <strong>of</strong> dorsal root ganglion neurons<br />
using a preparation with intact ganglia from newborn and adult<br />
animals. We avoided the use <strong>of</strong> cultured neurons for the<br />
determination <strong>of</strong> [Cl ] i because the expression <strong>of</strong> Cl<br />
transporters and, hence the equilibrium level <strong>of</strong> [Cl ] i , may<br />
change during culture. [Cl ] i in vivo may also be co-determined<br />
by the satellite glial cells which closely wrap each neuronal<br />
soma inside the ganglion (Hanani, 2005), and which are lost<br />
upon cell isolation. We utilized the Cl dependence <strong>of</strong> the<br />
fluorescence lifetime <strong>of</strong> MQAE to directly access [Cl ] i .We<br />
found that [Cl ] i levels were uniformly high in newborns. In the<br />
course <strong>of</strong> the first 3 weeks after birth, somatosensory neurons
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changed their mode <strong>of</strong> Cl handling, and most neurons lowered<br />
their [Cl ] i level to some extent. In adult dorsal root ganglia,<br />
[Cl ] i varied over a wide range <strong>of</strong> concentrations. The<br />
distribution <strong>of</strong> [Cl ] i levels among individual neurons indicated<br />
an E Cl range <strong>of</strong> 70 to 20 mV. Statistical analysis pointed to<br />
the presence <strong>of</strong> three distinct populations <strong>of</strong> neurons with [Cl ] i<br />
levels near 40, 60 and 80 mM, respectively. However, the<br />
interpretation <strong>of</strong> this finding requires further examinations. Our<br />
results suggest that Cl currents are inhibitory in some<br />
somatosensory neurons and excitatory in others.<br />
What is the molecular basis <strong>of</strong> this transition? Our PCR<br />
study shows that five members <strong>of</strong> the SLC12-family <strong>of</strong><br />
electroneutral Cl co-transporters (CCC6, KCC1, 3 and 4,<br />
NKCC1) show robust transcription at P1 which does not change<br />
during <strong>maturation</strong>. The mRNA levels <strong>of</strong> three other family<br />
members (CCC9, KCC2, and TSC) are lower, but persist during<br />
<strong>maturation</strong>. Our results are in accordance with in-situ<br />
hybridization studies on dorsal root ganglia from adult rats.<br />
Strong KCC1 and NKCC1 expression was detected with<br />
riboprobes, while KCC2 mRNA could hardly be detected<br />
(Kanaka et al., 2001). Moreover, using a combination <strong>of</strong> in situ<br />
hybridization and immunohistochemistry, Price et al. (2006)<br />
found that the NKCC1 mRNA displays 50% co-localization<br />
with markers <strong>of</strong> unmyelinated nociceptors (peripherin, CGRP,<br />
TRPV1) with diameters in the range <strong>of</strong> 15–35 mm. Only 10–<br />
20% co-localization was observed with a marker for the<br />
myelinated, low-threshold sensory neurons (N52 protein) <strong>of</strong><br />
somewhat larger size (25–55 mm). Interestingly, NKCC1<br />
mRNA was also detected in the satellite glial cells (Price<br />
et al., 2006), the second major cell population in the dorsal root<br />
ganglia. This observation points to a caveat in the interpretation<br />
<strong>of</strong> our PCR data, as they do not reveal from which cell type the<br />
SLC12 templates originated. Nevertheless, our observation that<br />
mRNA levels do not change during the course <strong>of</strong> the Cl<br />
transition argues against the notion that transcriptional<br />
regulation underlies the change in Cl <strong>homeostasis</strong> in<br />
somatosensory neurons.<br />
Our immunohistochemical results indicate that most<br />
somatosensory neurons are equipped with NKCC1 and, hence,<br />
are capable <strong>of</strong> accumulating intracellular Cl . This interpretation<br />
rests on the results obtained with two antibodies (one N-<br />
terminal, one C-terminal) and is consistent with similar reports<br />
from cat and rat dorsal root ganglia (Alvarez-Leefmans et al.,<br />
2001), as well as with the expression pattern <strong>of</strong> NKCC1 mRNA<br />
(Price et al., 2006). A recent study with different antibodies<br />
showed NKCC1 signals mainly or exclusively in the satellite<br />
glial cells (Price et al., 2006). To our knowledge, the antibodies<br />
in this study were not characterized as rigorously on dorsal root<br />
ganglia as the T4 and N-16 antibodies used here. The<br />
monoclonal T4 antibody stains somatosensory neurons and<br />
satellite glial cells, and it recognizes a single band <strong>of</strong> the<br />
appropriate size in a Western blot from dorsal root ganglia<br />
(Alvarez-Leefmans et al., 2001). Under our experimental<br />
conditions, staining <strong>of</strong> satellite glial cells is discernible, but<br />
staining <strong>of</strong> neurons is prominent. The polyclonal N-16 antibody<br />
appears to be specific as indicated by the preadsorption control.<br />
Together with the matching mRNA expression pr<strong>of</strong>ile (Price<br />
et al., 2006), the immunohistochemical data thus indicate<br />
that somatosensory neurons in situ express NKCC1. This<br />
result is in good agreement with the findings <strong>of</strong> Sung et al.<br />
(2000) who analyzed the reversal voltage <strong>of</strong> GABA-induced<br />
currents in NKCC1 knockout mice (Delpire et al., 1999). In<br />
NKCC1 / mice, the reversal voltage was shifted to more<br />
negative values, indicating a loss <strong>of</strong> Cl accumulation efficacy.<br />
The NKCC1 / animals also showed altered pain behavior,<br />
pointing to an important role <strong>of</strong> NKCC1 in nociceptor<br />
physiology (Sung et al., 2000; Laird et al., 2004; see also<br />
Granados-Soto et al., 2005).<br />
How is [Cl ] i lowered in most adult somatosensory neurons<br />
– in some cells even into the 10 mM range – without change in<br />
the SLC12 transcription pattern? Several recent reports support<br />
the hypothesis that the activity <strong>of</strong> <strong>chloride</strong>–cation cotransporters<br />
is altered by posttranslational modification. Two<br />
distinct mechanisms could be involved: (1) the NKCC1 and<br />
KCC proteins are regulated by phosphorylation (Gagnon et al.,<br />
2006; Giménez, 2006), and this regulation may determine the<br />
[Cl ] i level in each individual neuron. NKCC1 activity is<br />
increased by phosphorylation by the STE20-related protein<br />
kinases SPAK/OSR1 and WNK (Dowd and Forbush, 2003;<br />
Gamba, 2005; Moriguchi et al., 2005; Kahle et al., 2005; Vitari<br />
et al., 2006), while WNK kinases reduce Cl extrusion by<br />
KCC1-4 (De los Heros et al., 2006). Our data indicate that most<br />
somatosensory neurons are equipped with NKCC1 and the four<br />
KCC is<strong>of</strong>orms. Since all <strong>of</strong> these proteins are regulated by<br />
kinases, it is reasonable to speculate that the different [Cl ] i<br />
levels after <strong>maturation</strong> <strong>of</strong> Cl <strong>homeostasis</strong> result from different<br />
phosphorylation states <strong>of</strong> the Cl transporters. (2) The activity<br />
<strong>of</strong> the Cl exporters may depend on oligomerization. A recent<br />
study <strong>of</strong> the <strong>chloride</strong> transition in the auditory brain stem<br />
showed convincingly that the postnatal development <strong>of</strong> Cl<br />
extrusion correlates with oligomerization <strong>of</strong> KCC2 (Blaesse<br />
et al., 2006). Thus, KCC2 appears to be inactive as homomer in<br />
the neurons <strong>of</strong> newborn animals and to be turned active after<br />
dimerization. A similar <strong>maturation</strong> process may develop in the<br />
somatosensory system and may lead to enhanced Cl extrusion.<br />
We did not investigate contributions <strong>of</strong> Cl transporters that<br />
do not belong to the SLC12 family. Cl /HCO 3 exchangers <strong>of</strong><br />
the SLC26 family (Mount and Romero, 2004; Shcheynikov<br />
et al., 2006) may be contributing to [Cl ] i in vivo, or<br />
transporters from the SLC4 family (Romero, 2005). However,<br />
the Cl /HCO 3 exchanger is conceptionally associated with<br />
Cl uptake rather than Cl extrusion, in particular, because<br />
HCO 3 can be continuously generated in the cytosol by<br />
carbonic anhydrase (Rivera et al., 2005). In our experiments,<br />
we did not supply extracellular HCO 3 . It is, therefore, unlikely<br />
that the decrease <strong>of</strong> [Cl ] i in our experiments is caused by Cl<br />
extrusion through Cl /HCO 3 exchange. However, in the<br />
living animal, this transporter may contribute significantly to<br />
setting [Cl ] i levels in somatosensory neurons. Furthermore,<br />
our PCR analysis showed that thiazide-sensitive Na + /Cl cotransporter<br />
mRNA can be detected in dorsal root ganglia, albeit<br />
at a comparably low level as KCC2. It will be interesting to<br />
establish the cellular distribution <strong>of</strong> this protein within the<br />
ganglia.
Author's personal copy<br />
488<br />
D. Gilbert et al. / Int. J. Devl Neuroscience 25 (2007) 479–489<br />
What could be the physiological significance <strong>of</strong> the postnatal<br />
change in Cl <strong>homeostasis</strong> in somatosensory neurons? Recent<br />
studies on peripheral Cl effects indicate that depolarizing Cl<br />
currents amplify the primary signal in the sensory terminals <strong>of</strong><br />
nociceptors. Transduction in these neurons works without<br />
metabotropic amplification <strong>of</strong> the primary signal. The<br />
transduction channels, which are directly gated by heat,<br />
chemical or mechanical stimuli, are invariably Ca 2+ -permeable<br />
(McNaughton, 2004), and most somatosensory neurons express<br />
Ca 2+ -activated Cl channels (Kenyon and G<strong>of</strong>f, 1998; Lee<br />
et al., 2005; Currie et al., 1995). Stimulus-induced Ca 2+ -influx<br />
thus triggers Cl currents, and those neurons which accumulate<br />
Cl in their sensory endings are depolarized by Cl efflux<br />
(Granados-Soto et al., 2005). Accordingly, pain behavior can be<br />
induced in animal models by excitatory Cl currents in the skin<br />
(Ault and Hildebrand, 1994), and can be attenuated by<br />
experimental inhibition <strong>of</strong> Cl accumulation into the sensory<br />
endings (Willis et al., 2004; Laird et al., 2004). Based on these<br />
observations, Price et al. (2005) proposed that increased Cl<br />
accumulation into sensory endings <strong>of</strong> nociceptors promotes<br />
hyperalgesia. Our data suggest that the Cl dependence <strong>of</strong> the<br />
nociceptive response reflects the actual state <strong>of</strong> Cl accumulation<br />
in each individual nociceptive neuron. In general, the<br />
sensitivity <strong>of</strong> somatosensory neurons may be co-determined by<br />
the efficiency <strong>of</strong> Cl accumulation, which, in turn, is regulated<br />
by posttranslational modification <strong>of</strong> its Cl transporters.<br />
Interestingly, a recent study <strong>of</strong> [Cl ] i levels in axotomized<br />
mouse somatosensory neurons revealed that NKCC1 phosphorylation<br />
and a consequent rise <strong>of</strong> [Cl ] i from 31 to 68 mM is<br />
associated with peripheral nerve regeneration (Pieraut et al.,<br />
2007). Thus, a dynamic regulation <strong>of</strong> [Cl ] i levels may be<br />
involved in different cellular processes in somatosensory<br />
neurons, including signal transduction and growth.<br />
Taken together, this study demonstrates that Cl <strong>homeostasis</strong><br />
in somatosensory neurons develops during postnatal<br />
<strong>maturation</strong> into a state where [Cl ] i can be regulated<br />
individually in each neuron. Regulation does not affect the<br />
transcriptional level <strong>of</strong> electroneutral cation–<strong>chloride</strong> cotransporters,<br />
but may exert its control via posttranslational<br />
modification. The efficiency <strong>of</strong> Cl accumulation sets the level<br />
<strong>of</strong> [Cl ] i and may, hence, control the sensitivity <strong>of</strong> the adult<br />
sensory neuron.<br />
Acknowledgements<br />
We thank Dr. Joe Lynch (University <strong>of</strong> Queensland) for<br />
helpful comments on the manuscript. This work was supported<br />
by the Deutsche Forschungsgemeinschaft (Fr 937/6).<br />
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