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. 2005 Jan 13;563(Pt 3):843–854. doi: 10.1113/jphysiol.2004.074138

Increased persistent Na+ current and its effect on excitability in motoneurones cultured from mutant SOD1 mice

JJ Kuo 1,2, T Siddique 2,3, R Fu 3, CJ Heckman 1,2,4
PMCID: PMC1665614  PMID: 15649979

Abstract

Mutations in the enzyme superoxide dismutase 1 (SOD1) initiate a progressive motoneurone degeneration in amyotrophic lateral sclerosis (ALS). Transgenic mice overexpressing this mutation develop a similar progressive motoneurone degeneration. In spinal motoneurones cultured from presymptomatic mice expressing the glycine to alanine mutation at base pair 93 (G93A) SOD1 mutation, a marked increase in the persistent component of the Na+ current was observed, without changes in passive properties. This increase only enhanced neuronal excitability in high input conductance cells, as low input conductance cells exhibited a compensatory outward shift in the current remaining after Na+ blockade. High input conductance motoneurones tend to be large, so these results may explain the tendency of large motoneurones to degenerate first in ALS. Riluzole, at the therapeutic concentration used to treat ALS, decreased neuronal excitability and persistent Na+ current in G93A motoneurones to levels observed in the control motoneurones. Aberrations in the intrinsic electrical properties may be among the first symptoms to emerge in SOD1-linked ALS.

Amyotrophic lateral sclerosis (ALS) is usually a fatal neurodegenerative disease involving motoneurone degeneration. Patients with mutations in the enzyme superoxide dismutase 1 (SOD1) account for approximately 20% of all familial ALS cases (Deng et al. 1993; Rosen et al. 1993; Siddique & Lalani, 2002). Transgenic mice overexpressing a mutated human SOD1 gene develop a progressive neurodegeneration similar to SOD1-linked ALS in humans (Siddique, 1991; Gurney et al. 1994), with muscle weakness leading to paralysis (Kong & Xu, 1998). Additionally, spinal motoneurones from SOD1 transgenic mice acquire pathological features seen in patients, such as axonal spheroids (Dal Canto & Gurney, 1997) and fragmentation of the Golgi apparatus (Mourelatos et al. 1996). Results from studies using mutant SOD1 mice support the hypothesis that mutant SOD1 confers a toxic gain of function rather than an enzymatic loss of function. Despite nearly normal levels of SOD1 enzymatic activity, mutant SOD1 mice develop ALS, whereas SOD1 knockout mice do not (Gurney et al. 1994; Reaume et al. 1996; Wong et al. 2002).

The nature of the SOD1 gain of function has yet to be identified, but motoneurone vulnerability to excitotoxicity may be important. Studies have focused on glial glutamate transport, glutamate receptors and calcium buffering (Palecek et al. 1999; Beers et al. 2001; Cleveland & Rothstein, 2001; Rao & Weiss, 2004). However, intrinsic motoneurone excitability may also be a major contributor to excitotoxic vulnerability. Calcium enters the motoneurone not only through glutamate receptors during synaptic transmission, but also during each action potential through voltage-dependent Ca2+ channels (Powers & Binder, 2001). Thus, cells that generate a greater number of action potentials per unit of input are more excitable and likely to be more vulnerable to excitotoxicity.

Cultured motoneurones from presymptomatic mutant SOD1 mice, in fact, were characterized by enhanced intrinsic excitability, with a marked increase in the slope of the relation between the firing frequency (F) and injected current (I) (Kuo et al. 2004; Pieri et al. 2003). Many intrinsic motoneurone properties can affect the gain of the F–I function, including the afterhyperpolarization (AHP), Ca2+ currents and input conductance (Rekling et al. 2000; Powers & Binder, 2001). In addition, persistent currents (PCs) have a major impact on F–I gain (Hounsgaard et al. 1988; Hounsgaard & Kiehn, 1989; Bennett et al. 1998; Lee & Heckman, 1998). Although an L-type Ca2+ channel plays an important role in generating these PCs (Hounsgaard & Kiehn, 1989; Perrier & Hounsgaard, 2003), a persistent Na+ current (PCNa) is also important (Lee & Heckman, 1999; Li & Bennett, 2003). Moreover, PCNa is likely to be essential for spike generation during sustained inputs and thus should strongly influence F–I gain (Lee & Heckman, 2001). Riluzole, a drug that slows the course of ALS in mutant SOD1 mice (Gurney et al. 1996) and human patients (Bensimon et al. 1994), is in fact a selective blocker of PCNa at low concentrations (Urbani & Belluzzi, 2000).

We therefore tested the hypothesis that mutant SOD1 motoneurones have increased levels of PCNa. We further examined the role of PCNa. By pharmacologically inhibiting PCNa, we observed a marked decrease in excitability and PCNa. These results suggest that PCNa may play a direct role in motoneurone degeneration. Some of this work has been previously published in abstract form (Kuo et al. 2002).

Methods

All procedures were approved by the Northwestern University animal care and use committee.

Mice

Transgenic mice expressing the mutant (G93A) and wild-type human SOD1 gene were bred and maintained in barrier facilities. Mice overexpressing the G93A SOD1 mutation began to demonstrate clinical symptoms (tremors) at approximately 200 days old. Transgenic G93A mice represent an excellent model for the study of ALS, as many pathological and phenotypic symptoms resemble those observed in human patients (Mourelatos et al. 1996; Dal Canto & Gurney, 1997; Gurney, 1997; Kong & Xu, 1998; Bruijn et al. 2004). The control sample consisted of wild-type SOD1 and non-transgenic embryos from the human wild-type SOD1 mice. No statistical difference was observed in any parameter between these two samples, so they were combined as the control sample. Standard PCR techniques, as previously described, were used to identify the genotype of each embryo (Deng et al. 1993; Gurney et al. 1994). For part of the studies of riluzole inhibition, standard inbred C57BL6 (Harlan, Indianapolis, IN, USA) mouse embryos were used.

Cell culture

The spinal cord was removed, dissociated and cultured from embryonic mice at day 12–14, with some modifications (Anelli et al. 2000). After killing the pregnant mouse with an overdose of isoflurane followed by decapitation, each embryo was placed in an individual Petri dish containing cold Neurobasal-A medium (Invitrogen, Carlsbad, CA, USA). Each spinal cord was quickly removed and sliced into 400-μm slices. The dissociation and cell isolation of the spinal cord slices have been previously described (Levi et al. 1989). The dissociated cells were plated at approximately 130 000 cells cm−2 on glass coverslips coated with poly-d-lysine. The initial medium contained Neurobasal-A medium (Invitrogen), B27 Supplement (Invitrogen), 1% penicillin-streptomycin, 1 mml-glutamine and an additional 2 mg ml−1 glucose. The plating medium contained the initial medium plus 15% heat-inactivated horse serum. The plating medium was changed after 2 days in vitro to a serum-free maintenance medium containing the initial medium with 20 ng ml−1 nerve growth factors (Invitrogen). The maintenance medium was replaced every 3–4 days and cultures were used between 10 and 30 days in vitro.

Electrophysiology

Electrodes were typically 3–4 MΩ in resistance when filled with a solution containing (mm): potassium gluconate 145, CaCl2 0.1, EGTA 1.1, Hepes 5, MgCl2 2, and ATP-Mg2+ 5; with a pH of 7.3. Artificial cerebrospinal fluid (aCSF) contained (mm): NaCl 138.5, NaHCO3 28.8, NaH2PO4 1.1, KCl 3.3, MgSO4 1.6, CaCl2 2.8, glucose 11, picrotoxin 0.1 (Sigma, St Louis, MO, USA), 2,3-Dioxo-6-nitro-1,2,3,4, -tetrahydrobenzo[f]quinoxaline-7-sulfonamide disodium salt (NBQX) 0.01 (Tocris, Ellisville, MO, USA), strychnine 0.01 (Sigma) and D-(-)-2-Amino-5-phosphonopentanoic acid (AP5) 0.1 (Tocris); with a pH of 7.4 when bubbled with 95% O2–5% CO2. TTX was added to the aCSF as a 1 μm TTX solution. Riluzole was dissolved in DMSO and added to the aCSF as a 0.05% DMSO solution. Vehicle control experiments showed no differences. All aCSF and drug solutions were applied to the bath. Data were acquired at 10 kHz using a 1401 Plus (Cambridge Electronics Design) and digitally filtered off-line.

Whole-cell recordings

Whole-cell patch-clamp measurements were performed at room temperature using the Axoclamp 2A or Multiclamp 700A amplifier (Axon Instruments, Union City, CA, USA). Current–voltage (I–V) relations were generated using ramp voltage commands lasting 5 s. Voltage returned to baseline at the same rate as the ascending phase in all experiments. These slow ramps have been previously shown to provide a good estimate of the motoneurone steady-state I–V behaviour (Lee & Heckman, 1998). The relationship between action potential firing frequency and current was measured with triangular injected current waveforms, lasting 5 s each for the ascending and descending phases. Motoneurones were selected based on the presence of a multipolar cell body and a soma size greater than 25 μm in diameter (Carriedo et al. 1996).

Data analysis

Data were analysed off-line using IGOR Pro software (Wavemetrics, Lake Oswego, OR, USA). The input conductance of the cell was determined by fitting a linear regression to the I–V relation in its linear region, subthreshold to the voltage-sensitive currents (Powers & Binder, 2001). The leak conductance was subtracted from each waveform to produce the leak-subtracted I–V relation. An inward PC was readily apparent in each cell as a progressive downward deviation in the leak subtracted I–V function (Fig. 1C). This PC reflected the interaction between two basic components, which were revealed by TTX application. PCNa was measured as the difference between the raw I–V function and the function with TTX present (Fig. 1D). The difference between the zero level and the current remaining after TTX administration was defined as PCTTX-ins. The amplitudes of the total PC, PCNa and PCTTX-ins were measured as the integral of current with respect to voltage from 13 to 7 mV (Fig. 1C shaded region) hyperpolarized to the action potential voltage threshold, which was assessed from the first spike on the ascending phase of the F–I function. Our goal in referencing PCNa and PCTTX-ins measurements to spike voltage threshold was to focus these measurements to the voltage region where these currents have a strong impact on the genesis of rhythmic firing during the F–I function (Lee & Heckman, 2001; Powers & Binder, 2001).

Figure 1. Current response to a voltage ramp.

Figure 1

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A, the current response (top) from a voltage command (bottom) is shown with a single unclamped spike. Cell was held at −82 mV. B, the I–V relation (ascending ramp only) is shown for a pre-TTX (downward trace) and TTX trial (upward trace). C, leak-subtracted I–V relations are shown for pre-TTX and TTX trials. The shaded area represents the voltage region for PC integration (with respect to 0 pA, dashed line). D, leak-subtracted currents are shown for control (thin lines) and G93A (thick lines) cells. The downward currents are the subtraction of the TTX trial (PCTTX-ins) from pre-TTX and represents PCNa.

As in our previous study (Kuo et al. 2004), the F–I function provided an overall measurement of the neuronal steady-state excitability. The slope of the linear regression fitted to the ascending phase was defined as the F–I gain. The current thresholds were defined as the absolute current amplitude at the initial and final spike on the ascending and descending phases, respectively, of the current ramp protocol (see Fig. 3). The rate of rise of the action potential was calculated by dividing the time from spike threshold to action potential peak from this change in voltage. All other measurements for action potential properties were previously described (Kuo et al. 2004).

Figure 3. Firing response to a depolarizing current ramp command.

Figure 3

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A, the voltage response (top) to a current ramp command (bottom) is shown. The current thresholds for the initial and final spike are shown. B, the F–I relation for a control (○) and G93A (•) cell with the F–I gain is plotted for each cell.

Student's t test was used to test for a significant difference of the means between the G93A cell sample and the control cell sample. A probability of < 0.05 was accepted as significant. Only data with consistent resting membrane potentials, holding current and spike overshoot were used.

Results

Up-regulation of persistent Na+ currents

In all cells recorded, embryos were identified as positive or negative for containing the human SOD1 gene (either wild-type or G93A) using standard PCR techniques (Deng et al. 1993; Gurney et al. 1994). The G93A sample consisted of 33 cells. The control sample consisted of 27 cells (15 overexpressors of wild-type SOD1 and 12 non-transgenic from the wild-type SOD1 mice). As no significant differences were observed between the wild-type and non-transgenic samples, they were combined as the control sample.

The basic I–V functions resulting from the triangular commands are illustrated in Fig. 1. In some cells, a strong inward PC produced a negative slope region followed by one or more spikes probably initiated in the dendrites or axon, as the voltage commands showed little or no deviation due to a loss of clamp control (Fig. 1A). The addition of TTX eliminated the negative slope and spikes, indicating that the inward voltage-dependant conductance was PCNa and the spikes were dependent on Na+ rather than Ca2+. The leak-subtracted records (Fig. 1C) are shown as well as the subtraction of the TTX record from control to reveal PCNa (Fig. 1D). Note that PCNa and PCTTX-ins were larger in the G93A motoneurone (Fig. 1D).

Although the PCNa magnitude exhibited considerable scatter in both control and G93A cell samples, it nonetheless tended to be substantially larger in G93A than control motoneurones (P = 0.0001) (Fig. 2A). However, PCNa onset showed no significant differences (G93A, −60.7 ± 4.5 mV; control, −59.4 ± 5.4 mV; P > 0.3). As reported previously (Crill, 1996), PCNa activation began at a level approximately 10 mV depolarized with respect to the resting membrane potential; this activation voltage level was hyperpolarized with respect to the spike voltage threshold (Table 1). Overall, these results support the hypothesis that the SOD1 mutation is associated with an increase in the magnitude of PCNa.

Figure 2. Increased PCNa and PCTTX-ins in G93A motoneurones.

Figure 2

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A, PCNa was significantly larger in G93A motoneurones (•) than from control cells (○). The shaded histogram represents the number of G93A motoneurones and the unshaded histogram was the number of control cells: G93A, −129.49 ± 51.48 pA; control, −78.41 ± 43.32 pA. B, PCTTX-ins was significantly larger in G93A motoneurones (•) than from control cells (○): G93A, 45.77 ± 36.11 pA; control, 19.47 ± 53.35 pA. C, the PC was similar between G93A (•) and control cells (○), due to a larger outward PCTTX-ins offsetting the larger PCNa in the G93A cells: G93A, −83.71 ± 61.31 pA; control, −58.94 ± 45.10 pA. In each panel, the histogram was divided into 20-pA bins and the top symbols represent the mean ±s.d., *P < 0.05 and **P < 0.0001.

Table 1.

Motoneurone passive and action potential properties

Control G93A
All (n = 27) Low Gn (n = 15) High Gn (n = 12) All (n = 33) Low Gn (n = 16) High Gn (n = 17)
Input conductance (nS) 3.8 ± 2.0 2.1 ± 0.6 5.1 ± 1.6 3.7 ± 1.9 2.2 ± 0.7 5.0 ± 1.5
Resting Vm (mV) −70 ± 6 −68 ± 6 −73 ± 5 −69 ± 6 −71 ± 4 −67 ± 7*
AP threshold (mV) −49 ± 5 −49 ± 5 −50 ± 5 −48 ± 4 −46 ± 4 −50 ± 3
AP amplitude (mV) 76 ± 8 74 ± 8 78 ± 8 72 ± 10 70 ± 11 74 ± 9
AP half-width duration (ms) 2.0 ± 0.7 2.0 ± 0.6 1.9 ± 1.0 1.8 ± 0.6 2.2 ± 0.4 1.5 ± 0.5
Rate of rise (mV ms−1) 66 ± 20 58 ± 13 77 ± 22 59 ± 18 54 ± 18 63 ± 19
AHP (mV) 20 ± 5 22 ± 4 17 ± 4 21 ± 5 25 ± 4 17 ± 3
(n = 26) — (n = 14) (n = 32) (n = 15) —
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Both control and G93A samples were separated using a threshold of 3.25 nS (see Results) to measure the properties of all cells in the sample, low-input conductance (Gn), and high-input conductance cells in the respective cell types. No passive or action potential (AP) parameters were significantly different between the control and G93A motoneurones, with the exception of the high-input conductance G93A resting Vm (P < 0.05). This, though, was likely to be due to a larger number of cells in this sample exhibiting spontaneous firing and by excluding all tonically firing cells, the resting Vm was not significantly different. All values are mean ±s.d.

Changes in TTX-insensitive persistent currents

Although we intended to focus on PCNa, PCTTX-ins was also found to be significantly larger in the G93A sample (P < 0.05), though this difference (∼26 pA) was smaller than for PCNa (∼51 pA) (Fig. 2B). The larger outward current of the G93A motoneurones was surprising because this would normally be associated with a decrease in neuronal excitability. This difference in PCTTX-ins was probably not due solely to changes in an outward current. In about 22% (6/27) of the control cells, PCTTX-ins was net inward, compared to 6% (2/33) of the G93A cells (Fig. 2B). Thus PCTTX-ins probably consisted of a mixture of Ca2+ and K+ currents in most cells, suggesting that the net shift in the outward direction for PCTTX-ins in the G93A cells could be due to either an increased outward current or a decreased inward current.

Combined effects of persistent Na+ and persistent TTX-insensitive currents

Together, PCNa and PCTTX-ins defined the amplitude of the total PC. In nearly all G93A and control cells after leak subtraction, this PC was net inward (G93A, n = 32/33; control, n = 25/27). However, Fig. 2C illustrates that the PC magnitude was not significantly larger in the G93A motoneurones compared to control cells (P > 0.05). This lack of difference was due to the larger PCTTX-ins offsetting the larger PCNa in the G93A motoneurones.

Differences in excitability of low- and high-input conductance cells

The effects of the SOD1 mutation on PCNa and PCTTX-ins in relation to cell excitability were further studied by dividing the samples into low- and high-input conductance groups. Input conductance, which is proportional to soma size, is an especially important parameter for motoneurones (Powers & Binder, 2001), because it is a major determinant of their threshold for activation (i.e. recruitment) in normal motor behaviours (Henneman & Mendell, 1981; Binder et al. 1996). Moreover, large motoneurones and their neuromuscular junctions tend to degenerate before small cells in G93A SOD1 mice and, probably, ALS patients (Tandan & Bradley, 1985; Mohajeri et al. 1998; Frey et al. 2000). We used an input conductance of 3.25 nS to separate both samples (G93A, 16 low- and 17 high-input conductance cells; control, 12 low- and 15 high-input conductance cells).

We assessed the steady-state intrinsic excitability of the cell using the F–I function in response to a ramp of injected current (Fig. 3). In G93A motoneurones, the F–I gain was similar in both low- and high-input conductance cells, while control high-input conductance cells had lower F–I gains than their low-input conductance counterparts (Fig. 4A). As a result, the F–I gain in the low-input conductance samples was not significantly different between G93A and control motoneurones (P > 0.1), whereas the F–I gain was significantly larger in the high-input conductance G93A motoneurones (P = 0.01). The F–I gain was significantly higher in the entire G93A sample (G93A, 0.166 ± 0.087 Hz pA−1; control, 0.115 ± 0.040 Hz pA−1; P < 0.005).

Figure 4. Effect of input conductance on measured firing properties.

Figure 4

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A, the F–I gain for low-input conductance G93A (•) and control (○) and high-input conductance G93A (▴) and control (▵) motoneurones is shown. Only the high-input conductance sample had F–I gains significantly different. High-input conductance: G93A, 0.164 ± 0.082 Hz pA−1; control, 0.103 ± 0.034 Hz pA−1; low-input conductance: G93A, 0.167 ± 0.095 Hz pA−1; control, 0.130 ± 0.042 Hz pA−1. B, similar to the F–I gain, input conductance-related changes were observed in the current threshold for the initial spike. High-input conductance: G93A, 23.35 ± 49.49 pA; control, 69.38 ± 57.32 pA; low-input conductance: G93A, 21.33 ± 25.38 pA; control, 15.82 ± 19.61 pA C, input conductance-related changes were observed in the current threshold for the final spike. High input conductance: G93A, 43.96 ± 53.8 pA; control, 101.07 ± 65.98 pA; low-input conductance: G93A, 51.52 ± 39.68 pA; control, 30.73 ± 24.86 pA. A significant difference in the current thresholds was only observed in the high-input conductance G93A motoneurones. In each panel on the right side, the mean ±s.d. values are shown; *P < 0.05.

The current thresholds for the initial and final spike on the ascending and descending current ramp, respectively, exhibited a similar dichotomy with respect to input conductance. In the high-input conductance samples, the F–I functions for G93A motoneurones had a significantly lower initial spike current threshold (P < 0.05) and final spike current threshold (P < 0.02) compared to control motoneurones (Fig. 4B and C). F–I functions in low-input conductance G93A and control motoneurones, on the other hand, had similar initial spike (P > 0.5) and final spike current thresholds (P > 0.1) (Fig. 4B and C). These input conductance-related changes were further supported by an increase in spontaneously firing G93A motoneurones. In high-input conductance G93A motoneurones, 5/17 (29%) exhibited spontaneous firing, whereas none (0/15) of the high-input conductance control cells exhibited this behaviour. However, low-input conductance motoneurones showed similar values for control (3/12; 25%) and G93A (2/16; 13%) cells. In summary, in the high-input conductance G93A motoneurones, not only was F–I gain higher, but the current thresholds for the initial and final spikes were decreased.

Differences in persistent currents in low- and high-input conductance cells

The higher F–I gains and lower current thresholds in high-input conductance G93A motoneurones compared to control cells were explained by differences in PCNa and PCTTX-ins. The average values of PCNa magnitude for both low- and high-input conductance G93A motoneurones were significantly larger (P < 0.05 and P = 0.005, respectively) compared to the respective control sample (Fig. 5A). In contrast, PCTTX-ins was only significantly larger in the low-input conductance motoneurones (P < 0.05) (Fig. 5B). Thus, the input conductance-related changes in the F–I gain and current thresholds in G93A cells presumably occurred because the increased PCTTX-ins offset the increased PCNa in the low-input conductance cells whereas the lack of change in PCTTX-ins in the high-input conductance cells allowed the increased PCNa to enhance their excitability. The role of PCNa in influencing excitability in high-input conductance G93A cells was supported by a significant correlation between PCNa amplitude and F–I gain (r = 0.72, P = 0.001). Moreover, significant correlations between the onset of PCNa and current thresholds were also observed (initial spike threshold, r = 0.75, P < 0.001; final spike threshold, r = 0.76, P < 0.001) for the G93A high-input conductance samples. No significant correlations between PCNa and F–I parameters were observed in the low-input conductance sample, presumably due to the compensatory change of PCTTX-ins.

Figure 5. Effect of input conductance on persistent currents.

Figure 5

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A, G93A low-input conductance (•) and high-input conductance (▴) motoneurones have a significantly larger PCNa than their control counterparts (low-input conductance, ○; high-input conductance ▵). Low input conductance: G93A, −125.88 ± 42.21 pA; control, −80.97 ± 42.76 pA; high input conductance: G93A, −132.88 ± 60.04 pA; control, −76.36 ± 45.15 pA. B, the G93A low-input conductance motoneurones had a significantly larger PCTTX-ins than the control sample, while the high-input conductance samples had similar values. Low input conductance: G93A, 52.70 ± 40.28 pA; control, 5.91 ± 56.55 pA; high input conductance: G93A, 39.26 ± 31.52 pA; control, 30.32 ± 49.9 pA. C, only the high-input conductance samples had a significant difference in total PC. The increased PC in the G93A sample was consistent with an increased neuronal excitability in high-input conductance G93A motoneurones. Low input conductance: G93A, −73.18 ± 50.44 pA; control, −75.06 ± 41.88 pA; high input conductance: G93A, −93.63 ± 70.11 pA; control, −46.04 ± 44.71 pA. In each panel *P < 0.05 and **P = 0.005.

Relation between increased PCNa and cell injury

If increased PCNa contributes to cell degeneration in SOD1-mediated ALS, then drugs that suppress PCNa should be neuroprotective. Riluzole is presently the only FDA-approved. drug that significantly prolongs life in human ALS patients (Bensimon et al. 1994). In cortical cells, riluzole has recently been shown to effectively block PCNa and decrease neuronal excitability. Furthermore, this blockade occurs at concentrations low enough to be achieved via oral dosage in humans (about 1 μm; Urbani & Belluzzi, 2000). If suppression of PCNa indeed plays an important role in the neuroprotective effect of riluzole in ALS, this drug should also suppress PCNa at low concentrations in motoneurones. Figure 6A shows that this is the case, with 0.5 μm riluzole reducing PCNa in a non-transgenic (C57BL6 strain) motoneurone. In non-transgenic motoneurones, 0.5 μm riluzole decreased PCNa to approximately 82% of control (64–108%; n = 5) and PC to approximately 67% of control (50–114%; n = 5). The F–I gain was decreased to 84% of the control condition (67–98%; n = 5). This decrease in neuronal excitability, PC and PCNa, with the riluzole concentration used (0.5 μm), is unlikely to be due to an increase in outward, or hyperpolarizing, currents (Cao et al. 2002).

Figure 6. Inhibition of excitability and PCNa by riluzole.

Figure 6

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A, the I–V relations for PCNa are shown for the control condition (thick line) and in the presence of 0.5 μm riluzole (thin line). Riluzole decreased PCNa to approximately 69% of the control value. The I–V relation in the presence of TTX is also shown (dashed line). B, in the control condition (•), the F–I gain to the current ramp stimulus was 0.24 Hz pA−1. The addition of 0.5 μm riluzole (○) decreased the F–I gain to 0.174 Hz pA−1. C, the I–V relations for the control conditions (thick lines) and with 0.5 μm riluzole (thin, dotted lines) are shown with leak subtracted. The decrease in the PC (thin, dotted line) with riluzole was approximately 68% and 87% for PCNa (thick, dotted line).

Riluzole had similar effects on cultured G93A motoneurones. In fact, 0.5 μm riluzole decreased the F–I gain, PC and PCNa to levels observed in the control motoneurones (Fig. 6B and C). In these G93A motoneurones (n = 8), the F–I gain was reduced from 0.151 ± 0.051 Hz pA−1 to 0.084 ± 0.059 Hz pA−1 in the presence of 0.5 μm riluzole (Fig. 6B). This reduction (56%) in the F–I gain was similar to the difference observed between the entire G93A and entire control sample (G93A, 0.166 ± 0.087 Hz pA−1, n = 33; control, 0.115 ± 0.040, n = 27). The PC in the G93A motoneurones (n = 8) was reduced from −83.5 ± 50.4 pA to −46.4 ± 74.1 pA with 0.5 μm riluzole and PCNa (n = 6) from −140.2 ± 94.8 pA to −117.6 ± 90.9 pA with 0.5 μm riluzole (Fig. 6C). The magnitude of PCNa and PC of the G93A motoneurones in the presence of riluzole (PCNa,−117.6 ± 90.9 pA; PC, −46.4 ± 74.1 pA) was similar to that observed in the entire control sample (PCNa, −78.41 ± 43.32 pA; PC, −58.94 ± 45.10 pA).

Discussion

Although the G93A motoneurones were characterized by increased PCNa, PCTTX-ins was only significantly larger in low-input conductance motoneurones. A lack of a similar compensatory increase in PCTTX-ins in high-input conductance cells probably accounted for their increased excitability. These differential changes in excitability may account for the increased vulnerability of large motoneurones to degeneration in ALS (Tandan & Bradley, 1985; Mohajeri et al. 1998). Inhibition of PCNa and excitability by riluzole at therapeutic concentrations supports a role for PCNa and hyperexcitability in leading to premature cell death in the G93A SOD1 mice.

Ion channels involved in excitability changes

Because of the considerable variability in excitability and PCs, measurements in many cells were required. We thus sought to isolate only one type of current per cell, PCNa. A decrease in the transient Na+ current in transfected neuroblastoma cells with the G93A mutation has been reported (Zona et al. 1998). However, while decreased transient Na+ current itself would probably not account for the increased F–I gain, this decrease was associated with a depolarizing shift in the inactivation curve (Zona et al. 1998). If, as appears likely (Taddese & Bean, 2002), PCNa is very sensitive to the total Na+ current inactivation, a depolarizing shift could increase PCNa amplitude. Furthermore, the effect of riluzole in reducing PCNa is likely to involve a hyperpolarizing shift in the Na+ inactivation curve, therefore decreasing PCNa (Urbani & Belluzzi, 2000).

PCTTX-ins was probably a mixture of inward and outward currents. As in the present work, it will require a large sample size to accurately correlate each component. Based on the voltage region measured for PCTTX-ins, L-type Ca2+ currents, such as CaV1.3 channels, and SK, the calcium-dependent potassium current, are good candidates for the observed changes in PCTTX-ins (Rekling et al. 2000; Goldin, 2001; Powers & Binder, 2001; Xu & Lipscombe, 2001; Heckman et al. 2003).

Potential role of elevated PCNa in the genesis of ALS

Increased excitability may contribute to changes in oxidative stress (Hand & Rouleau, 2002), as well as altered mitochondrial (Heath & Shaw, 2002) and energy metabolism (Ellis et al. 2003), and perhaps a chronic state of energy source depletion. Additionally, increased firing rates could allow excessive Ca2+ entry and ALS-vulnerable motoneurones possess poor calcium buffering properties compared to ALS-resistant motoneurones (Palecek et al. 1999; Vanselow & Keller, 2000). A role for intrinsic excitability in motoneurone degeneration is also suggested by clinical data. ALS patients demonstrated an increased dose–response curve to transcranial stimulation of the motor cortex (Zanette et al. 2002), reflecting either increased excitability of corticospinal neurones or spinal motoneurones, or a combination of both.

The foregoing indicates that increases in intrinsic excitability could contribute to excitotoxicity and cell degeneration in ALS. The next step is to consider whether the increased excitability due specifically to aberrant up-regulation of PCNa plays a fundamental role. Two important results support this hypothesis. In ALS patients, motor axons exhibit properties consistent with increased PCNa (Mogyoros et al. 1998). Perhaps the most striking result concerns riluzole, which provides significant prolongation of life in human ALS patients and SOD1 mice (Bensimon et al. 1994; Gurney et al. 1996). Riluzole has a variety of actions, such as inhibition of glutamate release and enhancement of glutamate uptake (Doble, 1996; Dunlop et al. 2003). However, at therapeutic concentrations, riluzole also selectively and potently inhibits PCNa and decreases neuronal excitability (Urbani & Belluzzi, 2000). In a motoneurone, the persistent inward current (PIC), which is composed of PCNa and L-type Ca2+ current, also affects firing properties (Lee & Heckman, 1998; Heckman et al. 2003). The reduction in the F–I gain, PIC and PCNa in G93A motoneurones, due to a therapeutic concentration of riluzole (0.5 μm), to levels measured in control motoneurones, suggests that the neuroprotective action of riluzole may be directly related to the inhibition of PCNa and the resulting decrease in excitability.

It should be emphasized that an elevation of PCNa contributes to cell death and is not of course the sole factor. For example, elevated PCNa would increase the excitotoxic effects of (i) elevated glutamate in the spinal cord (Cleveland & Rothstein, 2001), (ii) high concentrations of Ca2+-permeable AMPA receptors on motoneurones (Vandenberghe et al. 2000; Van Damme et al. 2003) and (iii) poor motoneurone Ca2+ buffering capacity (Palecek et al. 1999; Vanselow & Keller, 2000).

Culture versus in vitro or in vivo

Adult turtle motoneurones grown in cell culture de-differentiate and lose their persistent L-type Ca2+ currents and, in the majority of cases, the ability to generate sustained rhythmic firing (Perrier et al. 2000). The motoneurones in this current study were cultured from the embryonic state and appeared to develop many of the characteristics of young motoneurones. All cells exhibited good rhythmic firing and a large amplitude PCNa. L-type Ca2+ currents did not appear to be present in most cells, as administration of TTX usually resulted in a net outward PCTTX-ins. However, we noted that several low-input conductance control cells did have a net inward PCTTX-ins, which may have been due to L-type Ca2+ channels. The absence of net inward currents in G93A motoneurones suggests that L-type Ca2+ currents may be suppressed in SOD1 mice as part of the mechanism of adaptation to increased PCNa in low-input conductance cells. This prediction needs to be evaluated in future studies using either slice preparations of juvenile mouse motoneurones (see Carlin et al. 2000) or, perhaps, an adult sacral mouse cord preparation based on an in vitro rat sacral cord preparation (see Li & Bennett, 2003).

Time course of onset of elevated persistent Na+ current

While it is unknown how culture development compares to the situation in vivo, the lack of differences in the passive cellular properties, consistent culture survival, and recordings well before the onset of symptoms (200 days old) suggest that these cultures represent a presymptomatic state. Therefore, the observed changes in PCNa and excitability may not be as large as other reported aberrations which may be examined just prior to overt symptom onset to end-stage.

The origin of the electrophysiological aberrations observed is presumed to be the motoneurones and their intrinsic properties. The isolation of the cultures to the spinal cord limited the effects of the strongest neuromodulatory input to motoneurones, the monoaminergic input from the brainstem (Rekling et al. 2000; Powers & Binder, 2001). In addition, all recordings were obtained with ionotropic synaptic transmission blocked. The absence of neuromuscular junctions in the spinal cultures suggests that the electrophysiological aberrations are initiated in the motoneurone, but it is possible that similar electrophysiological changes in motoneurones will occur as a compensatory mechanism for synaptic transmission failures at the neuromuscular junction (Balice-Gordon et al. 2000; Rich et al. 2002).

Significance of the difference in excitability of low- and high-input conductance cells

Motor outflow consists of two components, recruitment of motor units and rate modulation of already recruited motor units (Binder et al. 1996). If synaptic input is uniformly distributed among the pool of motoneurones innervating a muscle, then the motoneurone F–I functions are the only determinants of the recruitment and rate modulation pattern (Heckman &; Binder, 1993a, b). The initial spike threshold determines recruitment and F–I gain specifies rate modulation. Normally, because of the size principle of motor unit recruitment, type S motor units are called upon for early recruitment and long periods of steady firing, type FR motor units are fast, moderate force and moderate fatigue-resistant motor units recruited next, and type FF motor units are fast, high force and high fatigue-resistant motor units recruited last (Henneman & Mendell, 1981; Binder et al. 1996). Therefore, progressively larger forces are generated by recruitment of progressively larger, higher force and faster motor units. Type S motoneurones have both low-input conductances and small soma sizes, therefore may be expected to degenerate first. However, large motoneurones tend to degenerate before small motoneurones (Tandan & Bradley, 1985; Mohajeri et al. 1998). Our results may in part explain this paradox: the increase in excitability and PIC only occurred in high-input conductance cells.

The elevated excitability in high- but not low-input conductance G93A motoneurones constitutes a disruption in the normal hierarchy of electrical excitability. The normal sequence of recruitment, essential for good fatigue resistance in maintained motor behaviours, is critically dependent on the correlations between cell size, input conductance and F–I threshold. In fact, most ionotropic synaptic input systems tend to generate larger synaptic currents in high- rather than low-threshold motoneurones (Powers & Binder, 2001).

Predicted symptoms in SOD1 mice and human patients

The observed results could be used to predict symptoms that would occur in mutant SOD1 mice and in human ALS patients if PCNa is elevated and the initial spike current threshold is decreased before the onset of symptoms and overt motoneurone degeneration. The most striking of our results in this regard was the marked decrease in F–I threshold of the high-threshold units. Note that in Fig. 4B, both low- and high-input conductance G93A motoneurones have similar F–I thresholds, whereas in our control cells and in normal motoneurones (Binder et al. 1996), high input conductance, presumed type FR or FF motoneurones, have much higher F–I thresholds than low-input conductance, presumed type S motoneurones. Thus FF units would be predicted to be recruited during low force behaviours, such as posture or slow locomotion, which normally rely only on type S motor units. The FF units would in fact be an advantage for strength (and indeed such changes may mask the onset of muscle weakness) but they would produce undue fatigue in prolonged low force outputs. Thus an increase in fatigue and an increase in electromyographic (EMG) activity due to an increase in participating units may be very early signs of ALS.

A slow onset of increased FF excitability may convert the FF muscle fibres to slow twitch properties (Pette & Vrbova, 1999). While the excitability changes in FF motoneurones may be more difficult to detect, these changes would be readily apparent from measurements of recruitment order. Uniquely among CNS neurones, the firing patterns of motoneurones can be routinely assessed in human subjects because of the one-to-one relation between motoneurone firing and that of its muscle fibres (Powers & Binder, 2001). Thus, if motoneurones in vivo undergo the same changes in excitability as our cultured motoneurones, then instead of recruitment in order of increasing amplitude of motor unit twitches (measured in humans by an averaging technique; Milner-Brown et al. 1973), recruitment should be random.

The preferential increase in excitability of the high-input conductance motoneurones may, alternatively, be explained by differences in specific membrane resistivity. Shifts to higher input resistances, longer AHP durations and lower cell capacitance were observed in axotomized spinal motoneurones (Gustafsson & Pinter, 1984). These aberrations, thought to occur only in type FF motoneurones, indicated that axotomized FF motoneurones de-differentiate (Gustafsson & Pinter, 1984). The differences between our work and the results from the axotomized motoneurones (Gustafsson & Pinter, 1984) may reflect differences between in vitro and in vivo conditions. In addition to de-differentiation-induced aberrations, the emergence of axon-like processes from the distal dendrites may account for the observed electrophysiological changes in the high-input conductance motoneurones (Rose & Odlozinski, 1998; Rose et al. 2001; MacDermid et al. 2002; MacDermid et al. 2004). It is possible that in our cultures, the high-input conductance motoneurones developed these axon-like distal dendtritic processes that express Na+ channels, which could contribute to the observed hyperexcitability and increased PCNa. By staining for sodium channel subtypes, specifically those showing persistent kinetics, alterations in the distribution of sodium channels may be revealed (Goldin, 2001).

The aetiology of ALS is heterogeneous. By focusing on SOD1-linked ALS, the motoneurone abnormalities identified in this study can be used to generate predictions about recruitment order and EMG activity that can be tested on this distinct population of ALS patients. Moreover, recruitment order and EMG activity can be measured and tracked in individuals with the SOD1 mutation well before disease onset through disease progression.

Acknowledgments

Supported by the National Institute of Neurological Disorders and Stroke NS034382 (C.J.H.), NS37912 and NS021442 (T.S.), the Les Turner ALS Foundation (C.J.H., T.S.), Vena E. Schaff ALS Research Fund (T.S.), Harold Post Research Professorship (T.S.), Herbert and Florence C. Wenske Foundation (T.S.), Ralph and Marian Falk Medical Research Trust (T.S.), Abbott Labs Duane and Susan Burnham Professorship (T.S.).

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