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Diabetologia

, Volume 46, Issue 2, pp 213–221 | Cite as

Intra-axonal recording from large sensory myelinated axons: Demonstration of impaired membrane conductances in early experimental diabetes

  • Jasna Kriz
  • Ante L. PadjenEmail author
Article

Abstract

Aim/hypothesis

Diabetic neuropathy is accompanied by a range of positive (paresthaesia, dysesthaesia, pain) and negative (hypesthaesia, anesthaesia) neurological symptoms suggesting widespread alterations in axonal excitability. The nature and the mechanisms underlying these alterations in axonal excitability are not well understood. The aim of this study was to examine the extent of changes in membrane properties of an identified neuronal structure—the large myelinated sensory axons in early experimental diabetes in rats.

Methods

Intra-axonal microelectrode recordings from large sensory myelinated axons from the isolated sural nerve in short-term streptozotocin-induced diabetic rats were used to study membrane properties using standard current-clamp technique.

Results

In addition to decreased conduction velocity we found several differences in physiological properties of sensory axons from diabetic rats: decreased resting membrane potential, decreased single action potential amplitude associated with slower rate of rise and decrease in inward rectification associated with slight alteration in outwardly rectifying conductances indicating impaired potassium conductances.

Conclusion/Interpretation

These results extend previous indirect evidence that potassium and sodium ionic conductances, most notably the inward rectifier (IR, Ih), are altered in large sensory axons of diabetic rats. The depression of IR could underly clinical neurological findings in diabetic patients.

Keywords

Diabetic neuropathy streptozotocin rats sensory myelinated axons intra-axonal recording action potential inward rectification 

Abbreviations

AP

action potential

AP/2

AP half amplitude level

CV

conduction velocity

DAP

depolarizing afterpotential

DN

diabetic neuropathy

Ih

slow inward rectifier

RMP

resting membrane potential

Rp

peak resistance

Rss

steady state resistance

STZ

streptozotocin.

The peripheral neuropathy associated with diabetes is one of the most common polyneuropathies, and at least 50% of diabetic patients will develop a form of diabetic neuropathy within 25 years after diagnosis [1]. The pathogenesis of diabetic neuropathies and consequently their treatment remain elusive, in spite of a number of hypotheses advanced in the past decades. These hypotheses deal with several major areas, such as metabolic, ischaemia and oxidative stress, non-specific glycosylation, and disturbances in trophic factors [1, 2, 3, 4]. The histopathological findings of advanced diabetic neuropathy (DN) are characterized by axonal degeneration, demyelination and atrophy that are associated with highly diverse disturbances of peripheral nerve function [2, 5, 6]. Different positive and negative neurological signs associated with DN suggest modification in axonal membrane excitability. Indeed, one of the earliest detectable physical signs of early DN is a decrease in conduction velocity as signs of changes in excitability of peripheral nerves [7]. At the moment, little is known about the possible mechanisms involved in pathological changes in nerve function, however modification of axonal membrane conductances clearly is one of the factors involved [7, 7, 9].

Myelinated axons express a rich repertoire of ion channels selectively distributed in cellular compartments and serving the physiological role of myelinated axons to conduct nerve impulses [10, 11, 12]. Fast sodium channels located almost exclusively on nodal membrane are modulated by fast and slow outwardly rectifying potassium conductances located in the internodal membrane [11, 13, 15]. In addition, inward rectification induced by membrane hyperpolarization has also been shown in axons of the mammalian [16, 17, 18, 19] and amphibian [20] peripheral nervous system.

In mammalian myelinated axons the inward rectifier is activated relatively slowly by membrane hyperpolarization, it is permeable to both Na+ and K+ ions, blocked by extracellular application of Cs+ [11, 15, 16] and, unlike IKIR, also blocked by a specific antagonists ZD 7288 of Ih found in neuronal cell bodies [21, 22].

Axonal excitability is increased during the activation of this current, as a result of the depolarization that occurs as Na+ and K+ enter the axons. Therefore it is suggested that this conductance may maintain membrane potential during and after the high frequency firing that otherwise might result in excessive membrane hyperpolarization.

Previous extracellular studies on whole nerves showed that inward rectification is decreased in peripheral nerves exposed to hyperglycaemic hypoxia, a common complication of diabetes mellitus [23, 24, 25]. Recent findings by indirect electrophysiological methods indicate that inward rectification could be altered in human diabetic neuropathy [8] as well as in experimental diabetes [9]—(for a review see [7]).

In this study we examine rectifying and steady state properties of large myelinated axons from isolated sural nerve fibres in control and streptozotocin (STZ)-diabetic rats by intra-axonal recording and standard current-clamp technique. We report here that inward rectification and other ion conductances are impaired in large myelinated sensory axons of diabetic rats [26, 27].

Material and Methods

Experimental groups and diabetes induction

Experiments were carried out on STZ-treated Sprague Dawley male rats and age-matched control rats. Diabetes was induced in 3- to 4-week-old rats (weight 90–100 g) by three injections of STZ (45 mg/kg i.p. on three consecutive days). The rats were weighed regularly and their blood glucose concentration was measured (Medisense, Abbott Labs) in samples drawn from the tail vein. After 12 week of diabetes animals were hyperglycaemic, 24.2±0.98 mmol/l compared with 8.3±0.66 mmol/l (means±SE, n=10) with an approximate weight loss of 30% in diabetic animals.

The rats were killed by an overdose of anaesthetic (halothane). Sural nerves were quickly dissected out, pinned to the bottom of the wax-coated chamber with the insect needles and continually perfused with mammalian Ringer, containing in mmol/l: 127 NaCl, 1.9 KCl, 2.4 CaCl2, 1.2 KH2PO4, 1.3 MgSO4, 26 NaHCO3 and 10 glucose, saturated with 5% carbon dioxide and 95% oxygen (pH=7.4, temperature 22–25°C). All procedures were approved and carried out according to the McGill University Animal Care Committee.

Electrophysiology

Identification of axons and sampling procedure. Intracellular recordings were obtained from the isolated sural nerve. In keeping with our previous experiments on amphibian and mammalian nerves, [20, 28, 29] and the conduction velocity (>25 m/s at room temperature, as assessed by the latency between stimulus artefact and the rising phase of the action potential) all of the recorded axons belonged to a population of large myelinated axons. It is technically unlikely to obtain the stable intra-axonal recording from the axons that are less than 7 to 8 µm in diameter. In all our experiments at least two stable recordings were obtained from different axons from each sural nerve. Action potentials were evoked by brief 0.02 ms current pulses applied to the proximal trunk of the sciatic nerve via bipolar platinum electrodes at frequencies of 0.5 to 1.0 Hz. Axons were considered suitable for experiments if the resting membrane potential after stabilization was more negative than −65 mV (in control animals). Unlike amphibian, the depolarizing afterpotentials (DAPs) are observed only in 15% of sampled axons in mammalian axons [32, 33, 34, 35, 36] and therefore they were not studied. The microelectrode technique used in this study allows recording from undissected axons; it is likely that that such recordings reflect the excitability in vivo well [20, 30].

Microelectrode recording technique

Glass microelectrodes were prepared with a Brown-Flaming puller (Sutter Instruments, San Francisco, Calif., USA), filled with KCl (3 M) and had D.C. resistance 60 to 80 MΩ.

Microelectrodes were selected for their low noise and ability to pass less than or equal to 2 nA without rectification and were connected to Axoclamp 2B (Axon Instruments, Foster City, Calif., USA). An active bridge circuit allowed simultaneous current injection and recording through the same electrode ("current-clamp" technique). After capacity compensation the rise time (5–95%) of 50 mV voltage calibration pulse was 20 to 50 µs. This bandwidth allowed for appropriate bridge balance. Occasionally, bridge balance was checked independently by ensuring that the action potential overshoot remained constant [31]. After differential amplification (Axoclamp 2B, Axon Instruments) at 20 kHz following the low pass 8-pole Bessel filter set at 10 kHz, and a 16 bit A/D converter (ITC 16 Instrutech) with appropriate software (TIDA for Windows) records were stored on a computer for further analysis.

Differentiation of signals was done by computation of digital recording and data expressed as dV/dt.

Data analysis

Whenever appropriate, results were expressed as means ± standard error (SE). Statistical significance was assessed using one-way ANOVA followed by a Tukey HSD test. A p value of less than or equal to 0.05 was considered statistically significant.

Results

Resting membrane potential

Stable intra-axonal recordings described in this study were obtained from more than 50 randomly-impaled axons from isolated sural nerves of control rats and diabetic rats. Intracellular placement of the electrode was indicated by a sharp drop in the recorded potential (usually −65 to −70 in control axons) and the appearance of the brief action potential in response to stimulating pulse. Within 10 to 15 min the membrane potential stabilized. The average resting membrane potential was less negative in isolated axons from the diabetic rats (control, −73.5±0.57 mV vs. −70.8±0.92 mV in d, means ± SE, n=32) (Table <tablecite>1</tablecite>).

Characteristics of action potentials

As measured at half amplitude level (AP/2, Table 1) at resting membrane potential there was no difference in the action potential duration between the axons from control rats and those from diabetic rats. However, the action potentials recorded from myelinated axons of diabetic rats were smaller (Table 1; Fig. 1). This decrease in amplitude of action potential in axons of diabetic animals was associated with a decrease in the rate of the rising phase (depolarization) of action potentials (measured by differentiation and expressed as dV/dt; 486.04±28 vs. 388±23 V/s; n=25 and 23, respectively for control and STZ-treated rats, respectively; Fig. 1). There was no difference in the rate of the falling phase (repolarization) of action potential (Fig. 1B).
Table 1.

Resting and action potentials recorded in large myelinated in axons from control and STZ rats

RMP (mV)

AP (mV)

AP/2 (ms)

CV (m/s)

Control

−73.5±0.67

90.74±2.6

0.77±0.09

27.63±1.68

STZ

−70.8±0.92*

83.6±3.4*

0.79±0.03

17.86±0.77*

RMP = Resting membrane potential (Control, n=32; STZ, n=33), AP = action potential amplitude measured at resting membrane potential; AP/2 = half amplitude AP duration (Control, n=27; STZ, n=18), CV = conduction velocity (CV). Values represent means ± SE. Data marked in bold* type are statistically significant from controls, p ≤ 0.05. Intra-axonal recordings at 22–23°C

Fig. 1A–C.

Smaller action potential in sensory axon of diabetic rats. Intra-axonal microelectrode recording from sural nerves. Action potentials from control (A)and STZ-treated rats (B) sural nerves with corresponding first-order differential traces (dV/dt). (C) Average maximum and minimum dV/dt values recorded from control and STZ diabetic rats. Each column represents means ± SE (control n=22, diabetic n=25); *significantly different from control, p ≤ 0.05

Action potentials in myelinated axons are often followed by a depolarizing after-potential (DAP; Fig. 1A). The difference in DAP between control rats and diabetic rats as observed in Fig. 1 A is not significant.

When comparing the membrane potential and the rate of the rise of AP (dV/dt) there was a decrease in the correlation coefficient in diabetic rats compared with control rats, suggesting that the slower rate of rise in diabetic animals was not due to membrane depolarization but rather due to decreased voltage sensitivity of Na+ channel (Fig. 2).
Fig. 2A, B.

Correlation between dV/dt of rising phase of an action potential and membrane potential. Note the difference between the correlation coefficients indicating decreased voltage sensitivity of Na+ channels in diabetic animals (STZ rats; B) vs. control (A)

Conduction velocity

Conduction velocity was measured during stimulation of the distal trunk of the isolated sural nerve. It was calculated as the ratio between the latency of the stimulus artefact and the rising phase of an action potential and the distance between the stimulating and recording electrode. As expected, the average conduction velocity recorded from single myelinated axons from diabetic rats was reduced (17.9±0.8 vs. 27.6±1.7 for control rats, measured at room temperature, 23°C; Table 1).

Rectifying properties of axonal membrane

Intracellular injections of 200 ms depolarizing and hyperpolarizing current steps were used to examine the membrane properties of myelinated axons. The membrane voltage responses to current steps were characterized by several phases. In response to depolarizing steps a fast rising phase was followed by a slower rising response representing two outwardly rectifying conductances. As noted previously in mammalian and amphibian myelinated axons the action potential generation shows strong accommodation to depolarizing stimuli resulting in cessation of spiking (Fig. 3A). The difference in accommodation of action potential generation among experimental groups was not significant.
Fig. 3A, B.

Examples of characteristic voltage membrane responses to current steps (200 ms duration, 0.5 nA steps, not shown) and corresponding voltage/current plots recorded from single axon. (A) from control rat; (B) from diabetic rat. Note lack of sag in hyperpolarizing voltage responses in STZ-treated rats

In response to the hyperpolarizing pulses, membrane voltage responses of control axons showed characteristic upward "sag". (Fig. 3A). This sag was typically observed between 100 to 150 ms after the initiation of the current pulse and at membrane potentials 10 to 40 mV below RMP. It is generally accepted that this phenomenon reflects the activation of a slow inward current (Ih) in axons [10, 11]. Compared to the control rats, the axons of diabetic animals showed reduced upward sag, suggesting a decrease in inward rectification in these animals (Fig. 3, A vs B).

The voltage-current (V-I) relationship was constructed by plotting membrane potential at the peak of the voltage displacement and at the steady state near the end of the current step. The V-I relationship was strongly non-linear, reflecting the activation of more than one voltage-dependent conductance (Fig. 3A). The V-I plots from axons of diabetic animals were characterized by a decrease of time-dependent inward rectification (Fig. 3B).

The results were quantified by calculating the input resistance at different regions of the V-I relationships. In response to hyperpolarizing current pulses, at membrane potentials below −100 mV, two linear V-I relationships were used to calculate the input resistance: one obtained at the peak of responses (hRp, peak resistance) and the other at the steady state (hRss, for steady state resistance). Comparison of input resistances in sensory axons of diabetic animals in response to hyperpolarization showed an increase in hRss values, i.e. a decrease in inward rectification (35.3±2.6 MΩ, for control, vs. 45.0±5.0 MΩ, means ± SE, control n=17, STZ, n=21; Fig. 4A).
Fig. 4.

The average peak and steady state input resistance recorded during evoked hyperpolarization (hRp and hRss) and depolarization (dRp and dRss) in control and in the axons from STZ-diabetic rats. Each column represents means ± SE, (control, n=17, STZ n=21), * significantly different from control, p ≤ 0.05

Similarly, the input resistance to depolarizing stimuli was measured at two points: dRp, at 15 to 20 ms after pulse onset, and the steady state, dRss, 175 ms later (Fig. 4B). In response to depolarization myelinated axons of diabetic animals showed a slight increase in dRp values (15.93±0.79 MΩ, control, compared to 19.8±0.96 MΩ, for diabetic axons, control n=17, STZ=21) suggesting decreased activity of the fast outwardly-rectifying conductance (Fig. 4B).

Discussion

In this study using intra-axonal microelectrode recording we have shown decreased conduction velocity and altered membrane properties (Na, K and Ih conductances) of large myelinated sensory axons in short-term STZ-induced diabetic rats. Unlike previous studies that used either recording from single nodes of Ranvier or indirect measurements of axonal properties intra-axonal recording provides information about the single undissected axon which is especially relevant for understanding the complex functions of myelinated axon [10, 11], as discussed in the following sections.

Reduction of CV in experimental diabetic neuropathy

A decrease in nerve conduction velocity is an early feature of human diabetic neuropathy (cf. [3, 37]) and of experimental animal models (cf. [5]). Our results confirm that this abnormality is in large sensory myelinated axons.

The mechanisms underlying the slowdown of conduction velocity in early diabetes are not completely clear although there are several possibilities. The axon calibre is the most sensitive parameter affecting conduction velocity [38]. In chronic diabetes nerve conduction slowdown has been associated with neuroanatomical abnormalities [6, 39]. This is unlikely to be relevant for early diabetes, as recently shown in the diabetic rat [40].

We have shown a disparity between the unchanged axon calibre and decreased conduction velocity in peripheral nerves of transgenic mice with neurofilament H knock-out [35]. These findings point out that change in axonal membrane properties, such as reported in this study, are more likely to affect conduction velocity.

Na & K conductances are impaired in early animal diabetes

Early voltage clamp studies on nodal membrane indicated impaired permeability of Na channels [41]. Several possible explanations were proposed for this finding, such as (i) depolarization, (ii) defective ion channel function and (iii) a change in ion channel density and distribution.

(i) Depolarization of axonal membrane could result from Na,K pump blockade in diabetic animals (cf. [27, 42]) and/or suppression of inward rectifier, as reported in this study.

As expected, the intra-axonal recordings showed a decrease in amplitude of AP in large myelinated axons associated with a decrease in dV/dt of AP rising phase. However, this decrease is not only due to membrane depolarization but rather consistent with altered kinetics of sodium channel activation, as shown by the difference in correlation between the membrane potential and the rate of rise. The membrane depolarization of peripheral nerves in diabetic neuropathy has recently been discounted on the basis of the indirect but sensitive threshold tracking technique [43].

(ii) Na channel (and K or Ih channel) function can be affected by metabolic changes in diabetes through changed activity of intracellular second messengers and protein kinases. Recent studies in this laboratory indicate that the phosphorylation state of Na channels in peripheral nerves from diabetic animals could be affected, possibly because of changed activity of phophatases [44]. In addition to this postranslational changes of Na channels function it is possible that the diabetic state affects ion channel transcription. Thus studies in this laboratory show upregulation of a slow Na channel in peripheral nerves [45] and other data showed increased expression of the beta unit of the Na channel [46].

(iii) The molecular organization of the nodal region is not altered in BB-Wistar rat model of diabetes [47].

The responses of axonal membrane during depolarization associated with corresponding increase in input resistance, clearly suggest that fast K+ outwardly rectifying conductances are diminished in early experimental diabetes in agreement with previous studies by indirect techniques [7, 25].

An impairment of K conductances in diabetes is observed in other excitable tissues, such as the heart suggesting a generalized K conductance defect. It has been reported that the fast K+ channel activity is reduced by 50% at cytoplasmic pH of 6.8 as a result of enhanced anaerobic glycolysis [24, 48]. Decreased K channels could also explain our finding of membrane depolarization.

Inward rectification is reduced in early diabetic neuropathy

The most evident defect in diabetic sensory axons in our study was a attenuation of time dependent slow inward rectification associated with Ih. Clinical studies using the threshold electrotonus technique have provided evidence that Ih also occurs in human axons in situ [49], and that its effects on excitability are more pronounced in sensory than motor axons [50]. Recent data from peripheral nerves in human diabetic neuropathy indicate that axonal inward rectification might be diminished [8]. The abnormalities in diabetic patients were positively correlated with the age of patients and having neuropathy [8]. Using a similar technique on peripheral nerves in STZ-induced diabetic rats, another study also recorded a decrease in inward rectification that was reversed by an aldose reductase inhibitor treatment [9].

Functional implications

It is well recognized that experimental STZ diabetic rats develop neurological defects similar to those in human diabetic neuropathy: chronic pain as well as other signs of peripheral neuropathies, such as hyperalgesia to mechanical and chemical stimuli ([51, 52, 53]) and mechanical allodynia [54]. Therefore it is reasonable to expect that the mechanism of the defects is similar to human pathology. This study indicates that the large axons are also affected in early diabetes, in agreement with the clinical findings of impaired perception of vibration [5], that is commonly used to assess the function of large afferent Aβ fibers [55, 56].

Activation of Ih by hyperpolarization leads to depolarization that brings the membrane potential back towards the resting potential [11, 15, 16, 22]. Although the role of inward rectification in axons is not yet fully understood its activation prevents excessive hyperpolarization and possible conduction failure that might occur during high frequency firing [16, 17]. However, the effects of impaired Ih in diabetic neuropathy is minimized by the concomitant reduction in Na pumping (see above) and membrane depolarization.

The mechanism of the blockade of Ih in diabetic neuropathy is unknown. Besides its voltage-dependence, Ih is regulated by intracellular cyclic AMP concentration [22, 57, 58, 59] that is known to be decreased in diabetic nerves [60, 61].

In summary, our data show changes in nerve fibre conduction and excitability in early experimental diabetes that could provide the basis for some clinical symptoms related to diabetic neuropathy and possible targets for therapeutic intervention.

Notes

Acknowledgements

These studies were supported in part by grants from MRC, CDA and ALS. We thank Prof. K. Krnjevic for comments on an earlier version of the manuscript.

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Copyright information

© Springer-Verlag 2003

Authors and Affiliations

  1. 1.Department of Pharmacology and TherapeuticsMcGill UniversityMontréalCanada

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