Spikelets are non-synaptic events of small amplitudes (<30 mV) that are observed in intracellular recordings of many types of neurons (e.g. in thalamocortical neurons, Hughes et al., 2002; thalamic reticular neurons, Fuentealba et al., 2004; hippocampal interneurons, Zhang et al., 2004). Because of their spike-like appearance and all-or-none character, spikelets are considered to originate in action potentials (APs) generated in electrotonically distinct neuronal compartments, when currents from a remote AP influence the membrane voltage of the recorded compartment but do not suffice to initiate an AP there. As spikelets are typically measured in somatic recordings, the underlying APs might, in principle, occur in dendritic or axonal compartments within the same cell or in another cell coupled by gap junctions or ephaptically through extracellular fields (Figure 1).
As each of these mechanisms has different functional implications, it is important to determine the origin of spikelets to assess their potential computational role in a given system.
One factor that complicates (comparative) spikelet studies and contributes to the confusion about their origin is the many different names for spikelets that can be found in the literature. These alternative names, sometimes reflecting the presumed origin of spikelets, include the following: ‘IS spikes’ (IS: initial segment; Coombs et al., 1957), ‘fast prepotentials’ (FPPs; Spencer and Kandel, 1961), ‘short-latency depolarizations’ (Llinas et al., 1974), ‘d-spikes’ (d: dendritic; Wong and Stewart, 1992), ‘partial spikes’ (Zhang et al., 1998), ‘small spikes’ (Connors and Kriegstein, 1986), ‘third potentials’ (Kaplan and Shapley, 1984), and ‘ePSPs’ (electrical PSPs; Gibson et al., 2005).
The question of spikelet origin is resolved for some systems. For example, spikelets in cortical interneurons were found to result from electrotonic coupling by dendrodendritic and somatodendritic gap junctions, which increases the firing synchrony of interneurons and promotes generation and maintenance of network oscillations (Bennett and Zukin, 2004). In contrast, the origin of spikelets in cortical pyramidal neurons is still not settled. Virtually all possible spikelet mechanisms have been hypothesized to explain spikelet occurrence in these cells, but the experimental evidence is ambiguous.
In this article, we focus on spikelets in cortical pyramidal neurons. We first describe the properties of spikelets, noting that there are at least two qualitatively distinct spikelet types occurring in these cells. Then, we review the various mechanisms that can give rise to spikelets. We present theoretical considerations about spikelet properties generated by each of the possible mechanisms and compare them to experimental data from pyramidal neurons. We also discuss the functional implications of each type of spikelet.
Properties of spikelets in pyramidal neurons
At least two qualitatively different spikelet types have been observed in cortical pyramidal cells (Figure 2). The first spikelet type (Figure 2A, B) is characterized by relatively large amplitudes (typically in the range of 10 mV) and fast rise dynamics (max. dV/dt of 10–40 V/s). The decay is often, but not always, biphasic, with an initial faster phase (time constant <1 ms) followed by a slower phase (time constant >5 ms; Figure 2A, B right). These large-amplitude spikelets show an all-or-none behavior, and in a single cell there is usually one, rarely two, discrete amplitudes of spikelets (Schmitz et al., 2001; Crochet et al., 2004; Epsztein et al., 2010; Chorev and Brecht, 2012; Coletta et al., 2018). The generation of these spikelets is voltage-dependent, where somatic hyperpolarization suppresses the spikelets and somatic depolarization promotes the spikelet incidence (Crochet et al., 2004; Chorev and Brecht, 2012). Moreover, these large-amplitude spikelets are sensitive to sodium channel blockers, which suggests that they are actively propagating within the recorded cells (Schmitz et al., 2001; Crochet et al., 2004). This spikelet type occurs as a single event or in bursts with short inter-spikelet intervals of few milliseconds (Figure 2B). Interestingly, the large-amplitude spikelets can trigger somatic APs, which show a distinct initial rising phase (‘shoulder’) that fits the spikelet waveform (Epsztein et al., 2010). In CA1 pyramidal neurons in vivo, firing rates of these spikelets show spatial modulation with place fields virtually identical to the place fields of somatic APs (Epsztein et al., 2010). In presubicular head-direction cells, spikelets and APs from a single cell exhibit virtually identical head-direction tuning (Coletta et al., 2018).
A different type of spikelet was also found in both neocortical (Figure 2C; Scholl et al., 2015) and hippocampal (Figure 2D; Valiante et al., 1995) pyramidal neurons. These spikelets exhibit smaller amplitudes (typically in the range of 1 mV) and a brief time course (width at half-maximum amplitude <0.5 ms). Frequently, spikelets of several discrete amplitudes appear in a single cell, with inter-spikelet intervals similar to the inter-spike intervals. These small-amplitude spikelets occur independently of the somatic membrane potential or somatic APs. Accordingly, they are not suppressed by somatic hyperpolarization and were even observed superimposed on somatic AP bursts (Figure 2D). In CA1 pyramidal neurons, such spikelets were found during calcium-free-induced epileptic activity in slices (Valiante et al., 1995). Their occurrence correlated with population activity, as both were co-modulated by pH. Such brief spikelets were also reported in cat visual neocortex (Figure 2C; Scholl et al., 2015), where they shared several sensory selectivities with the APs, including orientation selectivity, receptive field location, and eye preference. However, binocular disparity tuning was typically not correlated between the APs and spikelets, and in half of the cells, the simple-cell/complex-cell receptive field properties did not match between APs and spikelets (Scholl et al., 2015).
The following sections review spikelet properties generated with the various mechanisms. We propose that the first type of spikelet (Figure 2A, B) fits best to axonal origin within a single cell; the second type of spikelet (Figure 2C, D) matches the properties of spikelets generated via ephaptic coupling to a neighboring cell.
Spikelets evoked by dendritic spikes
Historically, one of the first studies on spikelets in cortical neurons was carried out by Spencer and Kandel (1961). In 25% of units recorded in cat hippocampus in vivo, the authors observed fast events of small amplitudes (mean 5.9±2.4 mV), which were initiated approximately 10 mV below the usual AP firing threshold of these cells. These events were called ‘fast prepotentials’ (FPPs), because they only occurred spontaneously in the rising phase of APs. To study the FPPs in isolation, hyperpolarizing pulses had to be delivered to the soma during spontaneous discharges (Figure 3A, B). A ‘process of elimination’ was applied to deduce the origin of these events: As FPPs were present in rebound responses to intracellularly delivered hyperpolarization (Figure 3B), the authors reasoned that they probably originated within the impaled neurons. The decay of isolated FPPs appeared faster than a purely passive process (Figure 3C), so active currents were postulated in FPP generation. Next, as the antidromically evoked APs never showed FPPs, the authors proposed that FPPs might reflect dendritic spikes that are attenuated on their way to the soma. Finally, the presence of FPPs in response to stimulation of fibers projecting to the apical dendrite let the authors conclude that the FPPs originated in the apical dendritic tree. Because of the stereotypic appearance and small amplitudes of FPPs, the underlying dendritic spikes were supposed to occur in a single discrete area of the dendritic tree, separated by passive membrane from the soma. Functionally, FPPs of apical dendritic origin would act as a ‘booster’ for ‘otherwise ineffectual distal dendritic synapses’ (Spencer and Kandel, 1961).
Subsequent studies in the following decades indeed found that several neuron types including neocortical and hippocampal pyramidal cells (Golding and Spruston, 1998) have active dendrites capable of producing fast sodium spikes. However, these dendritic spikes occur in a graded manner (Golding and Spruston, 1998), so they are unlikely to result in all-or-none spikelets such as those described by Spencer and Kandel (1961). Moreover, dendritic sodium channels undergo slow inactivation (Mickus et al., 1999), so they do not support high-frequency firing as is typical for spikelets in vivo (e.g. Wong and Stewart, 1992; Crochet et al., 2004; Epsztein et al., 2010). Dual somatic and dendritic intracellular recordings demonstrated that dendritic spikes evoked in the distal apical dendrites of pyramidal neurons often fail to propagate to the soma (Spruston, 2008). However, these failed spikes appear as wide depolarizations at the soma (Figure 4; Golding and Spruston, 1998). Jarsky et al. (2005) discovered that the propagation of distal apical dendritic spikes is substantially facilitated by the activation of more proximal synapses. They observed that some somatically subthreshold responses exhibited spikelets of dendritic origin, yet the amplitude variability of these spikelets was not reported. Interestingly, distal apical inputs in CA2 pyramidal cells were shown to efficiently trigger dendritic spikes, which propagated reliably to the soma (Sun et al., 2014). Somatic hyperpolarization or a local TTX application revealed large and fast spikelets (amplitudes of 30–40 mV and max. dV/dt of 40–50 V/s), however, with graded amplitudes (Sun et al., 2014).
Not only apical but also basal dendrites of pyramidal neurons contain active conductances and fire dendritic spikes. Here, the resulting somatic spikelets appear rather slow (max. dV/dt up to 10 V/s) and have a distinct shape: the initial sodium spikelet is followed by a slower NMDA-receptor-dependent depolarization (Losonczy et al., 2008; Figure 5A). The latter, however, can be blocked by recurrent inhibition (Müller et al., 2012; Figure 5B). Nonetheless, repetitive initiation of dendritic spikes as well as AP backpropagation was found to cause inactivation of sodium channels in basal dendrites lasting for hundreds of milliseconds, resulting in attenuated dendritic spikes (Remy et al., 2009). Together, these properties of dendritic spikes enable basal dendritic branches to function as ‘independent processing units’ (Remy et al., 2009), where local synchronous synaptic input can trigger dendritic spikes, which evoke precisely timed AP output.
Even though dendritic spikes are commonly assumed to underlie spikelets in pyramidal cells (Wong and Stewart, 1992; Crochet et al., 2004), the graded nature of dendritic spikes and the inability of dendrites to fire at higher frequencies do not fit to the all-or-none spikelets occurring at high frequencies in these studies. Similar to the reasoning of Spencer and Kandel (1961), the dendritic origin of spikelets is often concluded from the observation that spikelets can be evoked by dendritic but not somatic inputs. The study by Stuart et al. (1997) might help to resolve this paradox: the authors performed triple dendritic, somatic, and axonal recordings in layer V pyramidal neurons and demonstrated that output APs were always initiated in the axon before the soma, even when a dendritic spike preceded the somatic AP (Figure 6). This suggests that spikelets evoked by dendritic inputs do not necessarily reflect dendritic spikes, but might instead stem from axonal APs that are triggered by the dendritic spikes.
Spikelets generated by axonal APs
In this section, we propose that large-amplitude (3–30 mV) all-or-none spikelets occurring with short inter-spikelet intervals in the soma of pyramidal neurons (Crochet et al., 2004; Epsztein et al., 2010; Coletta et al., 2018) can originate from axonal APs, even when they are evoked with orthodromic (dendritic) stimuli. We first present insights from pioneering studies and complement them with the recent knowledge about the axon initial segment (AIS) where AP initiation occurs.
Axonal APs and spikelets have been studied in various neuron types as early as in the 1950s. Coombs et al. (1955) examined AP propagation in motoneurons and found that an axonal AP evoked with a distal axonal stimulus and propagating antidromically toward the soma might fail to activate a somatic AP and appear as an all-or-none spikelet when the somatic membrane voltage is hyperpolarized (Figure 7A) or strongly depolarized (Figure 7B). The authors concluded that ‘there is the same failure of invasion, both when the membrane is heavily depolarized and the activation mechanism is continuously partially engaged, and when the membrane is hyperpolarized and the axonal currents are insufficient to depolarize the membrane to the extent of setting off the activation mechanism’ (Coombs et al., 1955). These observations hold also for pyramidal neurons, where somatic hyperpolarization is still a popular method to uncover and study antidromic axonal spikelets (Figure 7C; Hu et al., 2009).
Another way to generate antidromic spikelets is the so-called ‘two-shock technique’. Here, pairs of brief stimuli are delivered to the distal axon, resulting in a pair of somatic APs. Then, the interstimulus interval is decreased until the failure of the second somatic AP occurs and the underlying (all-or-none) spikelet is unveiled (Figure 7D; Kandel et al., 1961). This effect can be explained by a shorter relative refractory period of the axon as compared to the soma (Chen et al., 2010) and fits to the common occurrence of spikelets in bursts with short inter-spikelet intervals (Wong and Stewart, 1992; Crochet et al., 2004; Epsztein et al., 2010; Coletta et al., 2018). Consequently, the antidromically evoked spikelet is shaped by axial currents generated during the axonal AP propagation that result in a relatively fast and strong somatic depolarization: the spikelet.
Thus, antidromic axonal spikelets can easily be triggered by distal axonal stimulation, but it is not clear whether they also occur spontaneously in vivo. Besides a subpopulation of cortical interneurons, where antidromic APs and antidromic spikelets are generated in response to naturally occurring input patterns (Sheffield et al., 2010), antidromic spikelets – also called ‘ectopic’ – are typically reported in pyramidal neurons under various artificial or pathological conditions such as epilepsy (Avoli et al., 1998). These antidromic spikelets are characterized by an abrupt rise from the baseline without an underlying depolarization, and unlike orthodromic spikelets, they persist also during moderate somatic hyperpolarization. APs with these characteristics have been observed in in vitro models of gamma (Dugladze et al., 2012) and ripple oscillations (Bähner et al., 2011), but such ectopic APs were not found in recordings during ripple oscillations in vivo (English et al., 2014). However, antidromic spikelets would also result from axo-axonic coupling by gap junctions, which has been proposed for adult cortical pyramidal neurons (Schmitz et al., 2001; Hamzei-Sichani et al., 2007) and is reviewed in the section on electrotonic coupling.
For cortical pyramidal cells in vivo, inputs are usually considered to arrive at the soma orthodromically. It is not immediately evident how the mechanisms of antidromic spikelet generation might relate to orthodromic spikelets, i.e. spikelets evoked with dendritic synaptic inputs. Remarkably, Coombs et al. (1957) have shown in a series of experiments that ‘when an impulse is generated in a motoneuron by synaptic or direct stimulation [of the soma], there is the same two-stage invasion [of the soma] as with antidromic activation, though the [temporal] interval between the small-spike [spikelet] and the large-spike is much less than with antidromic invasion […], and it is more difficult to block the impulse between the two stages’. In these experiments, Coombs et al. could evoke somatic spikelets with direct (orthodromic) stimulation using the effects of somatic hyperpolarization and refractoriness. For example, somatic spikelets could be triggered by a brief somatic depolarization immediately followed by a hyperpolarizing pulse (Figure 8). This closely resembles the situation described by Crochet et al. (2004): ‘Cortical stimulation evoked a sequence of depolarization-hyperpolarizing potential; the early depolarization was crowned with an FPP [fast prepotential, i.e. a spikelet] when it reached the threshold for FPP generation’. The theoretical work by Michalikova et al. (2017) agrees with the above experimental results and demonstrates that the orthodromic inputs giving rise to spikelets are briefer and weaker than the inputs eliciting APs.
Interestingly, already Coombs et al. (1957) hypothesized that (orthodromic) somatic APs are initiated at the AIS where the firing threshold is about 10–20 mV lower than at the soma. This proposition was supported by early computational studies: Dodge and Cooley (1973) found that simulated motoneuron APs match the experimentally recorded waveforms when the AIS has a 10 mV lower threshold and 10 times larger sodium channel density than soma. Consequently, orthodromic spikelets might be viewed as (backpropagated) APs elicited at the AIS, which failed to trigger an AP at the soma. This failure does not happen as easily for orthodromic as for antidromic stimulation because the orthodromic stimulus depolarizes the soma closer to its threshold. However, the initial segment of vertebrate axons has been recently recognized as a distinct, complex, and plastic structure, involved in AP initiation and regulation of neuronal excitability. These recent findings support the possibility of axonal generation of spikelets and are reviewed in the information box ‘AIS – the site of AP initiation’.
AIS – the site of AP initiation
The AIS has been implicated in the AP generation already decades ago (Coombs et al., 1957). Additionally, early anatomical research identified its distinct ultrastructure, characterized by microtubule bundles and a dense granular layer underneath the plasma membrane (Palay et al., 1968), which distinguishes the AIS from the rest of the axon. Yet only technical advances in the past decade enabled to study the unique molecular composition of the initial segment in great detail (Rasband, 2010), providing the basis for further electrophysiological experiments and modeling work.
Since the pioneering work by Coombs and others, many independent studies have confirmed the AIS as the usual site of AP initiation in various neuron types, including hippocampal (Meeks and Mennerick, 2007) and neocortical (Palmer and Stuart, 2006) pyramidal cells. Further studies suggested that the AP threshold is lowest in the AIS because of its high density of voltage-gated sodium channels, up to 50 times higher than at the soma (Kole and Stuart, 2008). However, subsequent studies revealed a little difference between the sodium channel density at the AIS and soma (Fleidervish et al., 2010) and that APs were found to be initiated in the AIS even when its sodium channel density falls below that of the soma (Lazarov et al., 2018). Converging lines of evidence indicated that APs in cortical pyramidal neurons are initiated in the distal part of the AIS (Palmer and Stuart, 2006), where a distinct subtype of NaV channels was found to cluster (Royeck et al., 2008), activating at more hyperpolarized membrane potentials than somatic NaV channels (Colbert and Pan, 2002). Finally, Hu et al. (2009) demonstrated in layer V pyramidal neurons that the low-threshold NaV1.6 channels accumulate at the distal AIS and promote AP initiation. In contrast, the high-threshold NaV1.2 channels aggregate at the proximal AIS and are responsible for the backpropagation of the AP to the soma (Figure 9). The shift of the activation and inactivation curves between proximal and distal axonal locations was found to lie between 7 (Colbert and Pan, 2002) and 13 mV (Hu et al., 2009), which has been postulated to reflect a difference between the NaV1.6 and NaV1.2 channel subtypes (Hu et al., 2009).
In addition to the shifted activation and inactivation curves, the two Na-channel subtypes NaV1.2 and NaV1.6 were shown to differ in several other properties as well (Rush et al., 2005). The axonal NaV1.6 subunit was identified to generate larger persistent sodium current than the somatic NaV1.2 subunit (Rush et al., 2005). The axonal persistent current was found to be active already at resting potentials and to contribute to the low firing threshold of the AIS and to the rapid AP initiation (Fleidervish et al., 2010). Relevant for spikelet generation is also the finding that the axonal NaV1.6 subtype is able to better sustain high-frequency firing and conducts more current at high frequencies than the predominantly somatic NaV1.2 channel subtype (Rush et al., 2005). This might, at least partly, be caused by the slow, cumulative inactivation that was found in somatodendritic but not in axonal sodium channels (Mickus et al., 1999), predicting that high-frequency axonal firing is accompanied by high-frequency occurrence of somatic spikelets, as has been observed, for example, by Crochet et al. (2004) or Epsztein et al. (2010).
Interestingly, a recent study investigating AP initiation in NaV1.6-null pyramidal neurons demonstrated that the NaV1.6 subtype is not necessary for the lower firing threshold at the AIS compared to the soma (Katz et al., 2018). Rather, the authors suggest that the hyperpolarizing shift in the activation of axonal sodium channels might be a result of molecular interactions within the AIS. The hyperpolarizing activation shift has also been shown to undergo activity-dependent plasticity, co-occurring with synaptic long-term potentiation and decreasing the threshold of AP initiation (Xu et al., 2005). As an alternative explanation for the AP initiation at the AIS, Baranauskas et al. (2013) highlighted the role of neuronal morphology. Their study demonstrated that the AP threshold is lowest at the distal end of the AIS beyond the clustered sodium channels, where the capacitive load from the soma is the lowest.
Besides the NaV sodium channels, several potassium channel types are specifically localized in the axon and enriched at the AIS. The fast activating and slowly inactivating KV1 channels are colocalized at high densities with NaV1.6 subunits at the distal AIS but are rare at the soma. Kole et al. (2007) found that these potassium channels regulate the axonal AP waveform independently from the soma. Furthermore, the authors have shown that the AP width at the soma and the axon is modulated by different firing patterns: somatic APs become wider during high-frequency bursts, whereas axonal APs broaden during slow rhythmic activity (Kole et al., 2007). As the AP width at axon terminals controls the efficacy of excitatory synaptic transmission (Geiger and Jonas, 2000), this suggests that neuronal activity can be integrated in the axon independently from the soma.
The slowly activating and non-inactivating KV7 channels are likewise abundant in the AIS. They generate the subthreshold M-current, which diminishes neuronal excitability by increasing the AP threshold. In CA1 pyramidal neurons, the M-current has been found to suppress the intrinsic spontaneous firing (Shah et al., 2008). Moreover, M-current inhibition via cholinergic receptor activation exerts homeostatic effects on neuronal excitability: whereas acute M-current inhibition increases neuronal excitability, sustained M-current inhibition gradually reduces the excitability through a distal shift of the AP initiation zone (Lezmy et al., 2017).
The studies reviewed above imply that the variety of ion channels specifically targeted to the AIS provide powerful possibilities to set and regulate neuronal excitability and AP generation. Indeed, recently emerging evidence indicates that the neuron type-specific differences in firing properties and AP waveform can be largely explained by differences in the composition and organization of the AISs (Lorincz and Nusser, 2008; Kress et al., 2010). Moreover, it has been shown that the AIS is a highly plastic region, and its length as well as position can undergo activity-dependent plasticity (Grubb and Burrone, 2010; Kuba et al., 2010; Lezmy et al., 2017).
The highly specialized structure of the AIS, which can be activated and regulated independently from the soma, can promote the generation of orthodromic spikelets. These spikelets originate at the AIS like regular APs but fail to elicit a somatic AP (Michalikova et al., 2017). Such spikelets are characterized by relatively fast (max. dV/dt>10 V/s) and large (up to 20–30 mV) waveforms because of the large sodium currents evoked at the AIS. Unlike spikelets originating in dendritic spikes, axonal spikelets can occur at high frequencies because of the shorter refractory period of the axon in comparison to the soma. Finally, the generation of axonal (AIS) spikelets is dependent on the somatic membrane voltage due to the close proximity of the AIS.
Spikelets with these properties were reported in several in vivo studies (Figure 2A, B; Spencer and Kandel, 1961; Wong and Stewart, 1992; Crochet et al., 2004; Epsztein et al., 2010; Chorev and Brecht, 2012; Coletta et al., 2018), although only Coletta et al. (2018) implied an axonal origin of spikelets. It seems that the generation of spikelets upon dendritic inputs is an important factor misleading the interpretation. As discussed above and illustrated in Figure 6, the study by Stuart et al. (1997) directly demonstrated in neocortical pyramidal neurons that dendritic spikes can first initiate an AP at the AIS, which then triggers a somatic AP. Also recent studies in turtle pyramidal neurons (Larkum et al., 2008) and CA1 pyramidal neurons (Apostolides et al., 2016) suggest that spikelets triggered through dendritic stimulation might originate in axonal APs.
Orthodromically evoked spikelets of axonal origin have interesting functional consequences: the ability to generate output APs without firing an AP in the large somatodendritic compartments reduces the energetic costs of AP propagation (Ashida et al., 2007) and allows to control dendritic plasticity triggered by backpropagating APs (Spruston et al., 1995).
Spikelets resulting from electrotonic coupling by gap junctions
Another possibility for spikelet generation provides direct electrotonic coupling between pairs of neurons mediated via specialized structures called gap junctions. If two cells are coupled by such an electrical synapse, an AP occurring in one cell is transmitted through the gap junction and appears as a spikelet in the other cell.
Unlike chemical synapses, electrical synapses are reciprocal (though not necessarily symmetrical; Snipas et al., 2017), enabling passive current flow in both directions, depending on the potential gradient between the two connected compartments. The strength of electrotonic coupling, called coupling coefficient, is defined as the ratio of voltage change between the prejunctional and the postjunctional cell. The coupling coefficient depends on several factors: the junctional conductance, the transmitted voltage waveform (larger coupling coefficients for rectangular current injections than for AP waveforms), and the membrane properties of the postjunctional cell. The postjunctional membrane acts as a low-pass filter: the transmitted current first flows through the membrane capacitance, and as the capacitance gets charged, the current starts to flow through the membrane resistance. Consequently, slow fluctuations of the membrane potential are transmitted more effectively than fast signals like APs, which appear in the postjunctional cell as spikelets with slowed time courses and attenuated amplitudes (Figure 10A). Although the transmission of signals through gap junctions is immediate, an apparent delay can result from the time needed for capacitive loading of the postjunctional membrane to a detectable level (Bennett and Zukin, 2004).
In the mammalian brain, gap junctions were first demonstrated by Sloper (1972) as dendrodendritic or dendrosomatic close membrane appositions with a dense, seven-layered structure. Later work has revealed that gap junctions consist of clusters of channels directly connecting the intracellular space of the two coupled neurons such that ions and small metabolites can pass through. Vertebrate gap junction channels are composed of proteins called connexins. In neurons, connexin 36 is the predominant gap-junctional protein (Connors and Long, 2004), although other connexins are present as well: for example, Cx45 was found in retinal neurons (Li et al., 2008), and Cx26 occurs in neonatal excitatory cells of the neocortex (Su et al., 2017).
In the adult brain, gap junctions have been thoroughly demonstrated to connect hippocampal and neocortical interneurons of the same type (reviewed, e.g., in Galarreta and Hestrin, 2001). First, dual recordings identified coupled pairs, where a subthreshold current injection or an AP in one cell resulted in a voltage change or a spikelet waveform, respectively, in the other cell. Next, anatomical studies delivered ultrastructural evidence for the existence of dendrodendritic or dendrosomatic gap junctions as early as in the 1970s (Sloper, 1972). Finally, molecular studies revealed that interneuron gap junctions are composed of connexin 36. The coupling between interneurons was found abundant, but rather weak, and the spikelet waveforms resulting from AP transmission through these electrical synapses exhibit small amplitudes (typically <1 mV) and slow dynamics (Figure 10A). These weak dendrodendritic and dendrosomatic gap junctions in cortical interneurons were shown to promote neuronal firing synchrony, thereby significantly contributing to the generation and maintenance of network oscillations, for example, the hippocampal gamma (Traub et al., 2001) and ripple oscillations (Holzbecher and Kempter, 2018).
In contrast, controversy still accompanies the notion of electrical coupling between adult cortical pyramidal cells. Here, the evidence is mostly composed of dye coupling data (based on gap junctional permeability for small tracer molecules such as neurobiotin, biocytin, or Lucifer yellow) and pharmacological modulation of spikelet occurrence and waveform. Up to date, only few studies demonstrated direct electrical coupling in pairs of adult hippocampal (MacVicar and Dudek, 1981; Mercer et al., 2006) and neocortical (Wang et al., 2010) pyramidal neurons, and one study provided anatomical evidence for the presence of gap junctions between mossy fiber axons in the dentate gyrus (Hamzei-Sichani et al., 2007). Moreover, the protein underlying the electrical coupling in pyramidal neurons remains unknown.
The spikelet waveforms found in dual recordings of pyramidal cells are substantially larger (2–20 mV) and faster than the waveforms typical of interneuron spikelets (Figure 10B) and resemble the spikelet waveforms recorded in pyramidal neurons in vivo (Figure 2A, B). Furthermore, unlike interneuron spikelets, spikelets in pyramidal neurons are abolished when the sodium channels of the recorded neuron are blocked intracellularly with QX314, which suggests that these spikelets propagate actively in the putative postjunctional neuron. Consistent with the fast spikelet waveform and active propagation in the recorded neuron is axo-axonal coupling, which has been suggested in some studies (Schmitz et al., 2001; Wang et al., 2010), but not in others (Mercer et al., 2006).
This evidence of gap junctional coupling in pyramidal neurons is weakened by inherent issues associated with the methods used to demonstrate gap junctional coupling. First, the paired recordings are typically performed with sharp electrodes as these allow successive penetration of many neurons before they get clogged and have to be exchanged (Bennett and Pereda, 2006). However, sharp electrodes are prone to the so-called ‘shish-kebap artifact’, where the recording electrode would penetrate more neurons at the same time and could introduce artifactual coupling. This problem also affects dye coupling experiments, where further artifacts might occur because of, for example, dye leakage into the extracellular space that can be taken up by adjacent neurons (Jefferys, 1995). However, some of the methodological challenges were overcome in recent studies (Schmitz et al., 2001; Mercer et al., 2006; see Bennett and Pereda, 2006, for review).
Up to now, there is one study providing direct ultrastructural evidence for gap junctions in cortical excitatory neurons (Hamzei-Sichani et al., 2007). In thin-section transmission electron micrographs, the authors found altogether 10 close appositions of dentate granule axons called mossy fibers. Nonetheless, these putative gap junctions were missing the typical ‘submembrane densities’ and showed a pentalaminar instead of the typical heptalaminar structure. A further instance of a presumed axonal gap junction could be detected by freeze-fracture replica immunogold labeling using anti-Cx36 immunogold beads. However, it could not be determined whether the labeled axon was coupled to another axon or to a dendritic spine. Moreover, other studies did not find connexin 36 in pyramidal neurons (Hormuzdi et al., 2001; Pais et al., 2003).
Much more commonly, gap junctional coupling is inferred from modulatory effects of pH and pharmacology, although the effects of these manipulations are not specific to gap junctions (Connors and Long, 2004). For all connexins except Cx36, decreased intracellular pH (i.e. acidification) tends to close gap junctions, whereas increased intracellular pH (i.e. alkalization) opens gap junctions and strengthens electrical coupling (Connors and Long, 2004; González-Nieto et al., 2008). This behavior has been observed also for electrical coupling in pyramidal neurons (Schmitz et al., 2001)). In contrast, gap junctions formed by Cx36 respond in an opposite manner, opening upon acidification and closing upon alkalization (González-Nieto et al., 2008). However, pH levels have been shown to regulate not only gap junctions but various membrane channels as well (Chesler, 2003). Moreover, the physiological regulation of neuronal pH appears to be homeostatic: neuronal activity leads to acidosis, which in turn diminishes the excitability of neurons. Elevated pH has the opposite effect of increasing neuronal excitability (Chesler, 2003).
There are various pharmacological agents shown to modulate the strength of electrotonic coupling. These are chemically diverse and include long-chain alcohols such as heptanol or octanol, the anesthetic halothane, carbenoxolone, and mefloquine. However, most of these substances act non-specifically and have been shown to influence other physiological properties of neurons as well (Connors and Long, 2004). The specificity of carbenoxolone is controversial, with some studies reporting no influence on intrinsic neuronal properties (Schmitz et al., 2001), while others found reduction of various membrane conductances, increased AP threshold, or decreased input resistance (Rouach et al., 2003; Tovar et al., 2009). The quinine derivate mefloquine has recently gained interest as a specific and potent blocker of Cx36 channels, but also here some side-effects have been reported (Cruikshank et al., 2004). Yet it needs to be considered that if pyramidal cells are coupled at axonal sites, the transmitted AP is propagated actively in the axon of the postjunctional cell, and the propagation failure occurs close to the soma. Therefore, the pharmacological modulation of spikelet amplitude unlikely reflects not only a modulation of axo-axonal gap junction itself but also a change of some other neuronal property.
To address the question whether electrotonic coupling occurs in pyramidal neurons in vivo, Chorev and Brecht (2012) performed dual intra- and extracellular recordings of CA1 pyramidal neurons in anesthetized rats. The authors identified an extracellular AP waveform associated with, and slightly preceding, the onset of intracellular spikelets. Simulations of extracellular waveforms of APs and spikelets in compartmental models of pyramidal neurons showed that electrotonic coupling can in theory account for all aspects of the data. It would require gap junctions between the axons, in combination with a large (>several 100 µm) distance between the somata of the coupled cells, such that only the intracellularly recorded cell shapes the extracellular waveform (Michalikova et al., 2018). In contrast, paired recordings in hippocampal (Mercer et al., 2006) and neocortical (Wang et al., 2010) pyramidal neurons demonstrated electrical and dye coupling in cells with somata located very close to each other (Figures 11 and 12), but the close membrane appositions found at proximal somatodendritic sites did not show any ‘distinctive structures indicative of a gap junction’ (Figure 11; Mercer et al., 2006).
In short, only few in vitro studies have shown directly, i.e. through dual recordings of coupled neurons, that spikelets in cortical pyramidal neurons can result from electrotonic coupling, and the anatomical evidence for gap junctions is scarce. Theoretical as well as some experimental studies have suggested an axonal coupling site, which could account for the relatively large amplitudes, fast time course, and active propagation of these spikelets in the postjunctional cell (Traub et al., 1999; Schmitz et al., 2001; Wang et al., 2010). Theoretical studies proposed that axo-axonal coupling of pyramidal neurons could underlie the generation of high-frequency oscillations such as hippocampal ripples (Traub et al., 1999), which is supported by experimental studies showing that in vitro ripples can occur without GABA-A receptors (Draguhn et al., 1998; Nimmrich et al., 2005). However, recent experimental studies indicate that also local inhibitory synaptic interactions can give rise to the ripple oscillation in vitro (Schlingloff et al., 2014) as well as in vivo (Stark et al., 2014). Spikelets generated by axo-axonal coupling are similar to spikelets evoked antidromically within a single neuron, as the AP transmitted through the gap junction propagates antidromically in the postjunctional axon and the spikelet emerges as a propagation failure at the soma. This similarity in mechanism, along with the inherent difficulty to prove gap-junction coupling, obscure the ultimate answer to the question whether gap junctions are present in adult pyramidal neurons.
Spikelets produced by ephaptic coupling
Ephaptic coupling is a form of electrical coupling between two cells without a specialized connection like a synapse or a gap junction. The term ‘ephapse’ (from Greek εϕαπτω – to touch) was coined by Arvanitaki (1942) to describe ‘the locus of contact or close vicinity of the active functional surfaces’. Such a close apposition of neuronal compartments enables transmission of electrical signals from one cell to another via extracellular electric fields. Here, we follow the seminal work by Jefferys (1995) and distinguish ephaptic coupling from population field effects. For the latter phenomenon, synchronized activity of many neurons generates large extracellular fields, which influence the membrane voltage of the entire neural population located within the reach of the field (Konnerth et al., 1984; Dudek et al., 1986). Indeed, the stereotypical spike-like waveforms of spikelets indicate that spikelets originate from individual APs. So when an AP is triggered in one cell, a spikelet waveform might be visible in another cell that has a process located in close proximity to the firing cell.
Unlike the ‘resistive coupling’ by gap junctions that results in slow, low-pass filtered spikelets, the nature of ephaptic AP transmission is capacitive: there is no transmembrane current flow, but the charge is redistributed on the intra- and extracellular surfaces of membranes (Valiante et al., 1995; Vigmond et al., 1997; Weiss and Faber, 2010). Consequently, the AP waveforms are high-pass filtered, and ephaptic spikelets appear brief, typically briefer than the underlying APs (Vigmond et al., 1997). The hallmark of ephaptic spikelets is a fast decay – on the same order as the rising phase – and a frequently observed biphasic shape (i.e. a depolarizing phase followed by a hyperpolarizing phase), which clearly distinguishes ephaptic spikelets from all other types of spikelets.
Such brief spikelets were observed in CA1 pyramidal neurons in vitro during calcium-free-induced epileptic activity where in every cell the amplitudes of spikelets occurred in two to four well-defined clusters (Valiante et al., 1995; Figure 2D). Another example of putative ephaptic spikelets is provided in the study by Scholl et al. (2015), which found that spikelets in cat visual cortex in vivo shared some, but not all, sensory selectivities with the APs recorded in the same cell (Figure 2C).
Amplitudes of these somatically recorded spikelets were several millivolt large (1–6 mV), which agrees with theoretical and modeling predictions for transmembrane voltage changes due to ephaptic AP transfer from a soma to a neuronal cable (Holt and Koch, 1999). However, Vigmond et al. (1997) noted that in a passive model of a CA3 pyramidal neuron, the amplitudes measured intracellularly were an order of magnitude smaller (<0.1 mV) than the induced transmembrane potentials. Holt and Koch (1999) pointed out that ephaptically generated transmembrane potentials do not spread electrotonically ‘unless there are active channels at the location of the ephaptic depolarization’. Fast sodium currents active at subthreshold potentials could, in principle, boost the intracellular amplitudes of spikelets. Vigmond et al. (1997) alternatively proposed that intracellular spikelet amplitudes of several millivolts might be achieved by synchronized firing of several close-by neurons. This is conceivable for epileptic activity (Valiante et al., 1995) but rather unlikely to occur under physiological in vivo conditions (Scholl et al., 2015).
In general, ephaptic interactions are weak even for cells that are very close (3 nm apart in the model of Vigmond et al., 1997) because the AP waveform is transmitted through the low-resistance extracellular medium. Consistently, increased extracellular resistance has been shown to promote ephaptic coupling: Jefferys (1995) reviewed experiments with squid giant axons, where even APs could be evoked in an ephaptically coupled axon if the two nearby axons were immersed in mineral oil, which acts as an insulator and thus increases extracellular resistance. The physiological extracellular resistance is largest in brain regions with densely packed cells and restricted extracellular space like in rat hippocampus, especially in the CA1 cell body layer, which has double the resistivity of the surrounding layers (Gold et al., 2006). Moreover, the extracellular space is not constant over time but shrinks with intense neuronal activity that results in tissue swelling (Fox et al., 2004; Weiss and Faber, 2010). This might explain the occurrence of ephaptic spikelets in CA1 pyramidal neurons under epileptic conditions. However, neocortical tissue is less densely packed, and the in vivo activity is incomparable to epileptic states. So it is not immediately clear how ephaptic spikelets of several millivolts in amplitude can be generated in neocortical cells as observed by Scholl et al. (2015).
Cable theory posits that the voltage change induced by ephaptic coupling is smaller in thinner cables like axons than in thicker cables like dendrites (Holt and Koch, 1999). In contrast, Han et al. (2018) found ephaptic coupling between AISs of cerebellar Purkinje cells, which promotes firing synchrony in pairs of these cells. This coupling is enabled by the high density of sodium channel at the AIS, such that the generated extracellular potentials are large enough to activate sodium channels in nearby axons.
Thus, further theoretical studies are needed to examine ephaptic coupling in active models and to identify factors that might result in relatively large spikelet amplitudes in the millivolt range. Future studies should also assess the effect of activity-dependent tissue swelling on ephaptic coupling and the occurrence of spikelets (Jefferys, 1995; Weiss and Faber, 2010). Finally, the potential functional role of ephaptically induced spikelets in pyramidal neurons needs to be understood. Similar to population field effects, ephaptic coupling can synchronize the firing of close-by neurons but without the influence on the whole network (Han et al., 2018). However, it is also possible that ephaptic spikelets in pyramidal neurons are an epiphenomenon – and, at best, an indicator – of the network state.
We have reviewed the various spikelet-generating mechanisms with the aim to understand the origin of spikelets in pyramidal neurons. Table 1 provides an overview of the different mechanisms including spikelet properties and functional implications of each of the mechanisms. We note that at least two qualitatively different all-or-none spikelets appear in the experimental literature. One spikelet type is defined by small amplitudes and a very brief time course (width at half-amplitude<0.5 ms; Valiante et al., 1995; Scholl et al., 2015), which fits well to theoretical predictions of waveforms transmitted ephaptically through extracellular fields. More reports, however, are associated with the other spikelet type, which exhibits relatively large amplitudes (up to 30 mV) and fast rise times (max. dV/dt of 10–40 V/s; Crochet et al., 2004; Epsztein et al., 2010; Chorev and Brecht, 2012; Coletta et al., 2018). Several lines of evidence point to an axonal origin of these spikelets, especially the short inter-spikelet intervals, its large and fast waveform, its dependence on membrane polarization, and active conductance within the recorded neuron. Such axonal spikelets can be generated either in a single cell or in pairs of cells coupled with axonal gap junctions. Albeit the existence of axo-axonal gap junctions is controversial, more work is needed to definitely distinguish between these two mechanisms. The present review demonstrates that spikelets of different origin might occur within a single system and provides information that can help to elucidate the origin of spikelets also in other systems where this question is still not resolved.
Overview of the spikelet-generating mechanisms.
|Spikelet mechanism||All-or-none spikelets||Spikelet properties||Functional relevance in pyramidal neurons||Selected experimental and theoretical studies|
|Dendritic spikes, apical||No||1. Graded amplitudes|
2. No spikelet bursts
3. In CA1 pyramidal neurons: Wide and slow depolarizations at the soma
4. In CA2 pyramidal neurons: Large (30–4 mV) and fast (dV/dt of 40–50 V/s) spikelets
|Boosting of distal apical inputs||Experiment: Golding and Spruston (1998); Jarsky et al. (2005); Sun et al. (2014)|
Theory: Traub and Llinas (1977)
|Dendritic spikes, basal||No||1. Graded amplitudes|
2. No spikelet bursts
3. Slow spikelets (dV/dt<10 V/s)
4. Spikelet can be followed by NMDA-depolarization plateau
|Independent information processing at individual dendritic branches||Experiment: Losonczy et al. (2008); Remy et al. (2009); Müller et al. (2012)|
Theory: Traub and Llinas (1977)
|Axonal APs, antidromic||Yes||1. Large (3–30 mV) and fast (max dV/dt 10–40 V/s) spikelets|
2. Spikelets occur in bursts with short inter-spikelet intervals
3. Spikelets are abolished by intracellular sodium channel blockers
4. Spikelet decay is faster than purely passive decay
5. Spikelets arise abruptly from the baseline, without prior depolarization
6. Somatic threshold of spikelets is highly variable
7. Spikelets are not abolished by moderate somatic hyperpolarization
|Indication of epileptic discharges||Experiment: Coombs et al. (1955); Avoli et al. (1998); Schmitz et al. (2001); Hu et al. (2009)|
Theory: Dodge and Cooley (1973); Michalikova et al. (2017)
|Axonal APs, orthodromic||Yes||1. Large (3–30 mV) and fast (max dV/dt 10–40 V/s) spikelets|
2. Spikelets occur in bursts with short inter-spikelet intervals
3. Spikelets are abolished by intracellular sodium channel blockers
4. Spikelet decay is faster than purely passive decay
5. Spikelets arise from a preceding (synaptic) depolarization
6. Somatic threshold of spikelets is depolarized w.r.t. resting membrane potential
7. Spikelets are abolished by somatic hyperpolarization
|Energy saving; possibility to regulate dendritic plasticity caused by backpropagated APs||Experiment: Coombs et al. (1957); Crochet et al. (2004); Epsztein et al. (2010); Chorev and Brecht (2012); Coletta et al. (2018)|
Theory: Michalikova et al. (2017); Michalikova et al. (2018)
|Gap junctions, somatodendritic||Yes||1. Amplitude and max dV/dt of spikelets depend on the strength of the gap junction coupling|
2. Spikelets are low-pass filtered APs (‘resistive coupling’)
3. Spikelets are not abolished by intracellular sodium blockers
|Firing synchrony that promotes generation and maintenance of network oscillations||Experiment: Mercer et al. (2006); Wang et al. (2010)|
Theory: Vigmond et al. (1997); Michalikova et al. (2017); Michalikova et al. (2018)
|Gap junctions, axonal||Yes||1. Amplitude and max dV/dt of spikelets independent of the strength of the gap junction coupling|
2. All properties of antidromic axonal spikelets apply here as well
|Generation of hippocampal ripple oscillations||Experiment: Schmitz et al. (2001); Hamzei-Sichani et al. (2007); Wang et al. (2010)|
Theory: Traub et al. (1999); Michalikova et al. (2018)
|Ephaptic coupling||Yes||1. Spikelets are high-pass filtered APs (‘capacitive coupling’)|
2. Brief spikelets with fast decay
3. Spikelet amplitudes of 1–6 mV
4. Often biphasic spikelets: depolarization followed by hyperpolarization
5. Often several clusters of spikelets with different shape and amplitude within a single cell
|Indication of in vitro epileptic activity (calcium-free); firing synchrony of neighboring neurons||Experiment: Valiante et al. (1995); Scholl et al. (2015)|
Theory: Jefferys (1995); Vigmond et al. (1997); Holt and Koch (1999); Weiss and Faber (2010)
Apostolides, P.F., Milstein, A.D., Grienberger, C., Bittner, K.C., and Magee, J.C. (2016). Axonal filtering allows reliable output during dendritic plateau-driven complex spiking in CA1 neurons. Neuron 89, 770–783.
Ashida, G., Abe, K., Funabiki, K., and Konishi, M. (2007). Passive soma facilitates submillisecond coincidence detection in the owl’s auditory system. J. Neurophysiol. 97, 2267–2282.
Avoli, M., Methot, M., and Kawasaki, H. (1998). GABA-dependent generation of ectopic action potentials in the rat hippocampus. Eur. J. Neurosci. 10, 2714–2722.
Bähner, F., Weiss, E.K., Birke, G., Maier, N., Schmitz, D., Rudolph, U., Frotscher, M., Traub, R.D., Both, M., and Draguhn, A. (2011). Cellular correlate of assembly formation in oscillating hippocampal networks in vitro. Proc. Natl. Acad. Sci. USA 108, E607–E616.
- Export Citation
Bähner, F., Weiss, E.K., Birke, G., Maier, N., Schmitz, D., Rudolph, U., Frotscher, M., Traub, R.D., Both, M., and Draguhn, A. (2011). Cellular correlate of assembly formation in oscillating hippocampal networks in vitro. Proc. Natl. Acad. Sci. USA)| false 108, E607–E616. 10.1073/pnas.1103546108
Baranauskas, G., David, Y., and Fleidervish, I.A. (2013). Spatial mismatch between the Na+ flux and spike initiation in axon initial segment. Proc. Natl. Acad. Sci. USA 110, 4051–4056.
Bennett, M. and Zukin, R. (2004). Electrical coupling and neuronal synchronization in the mammalian brain. Neuron 41, 495–511.
Chen, N., Yu, J., Qian, H., Ge, R., and Wang, J. (2010). Axons amplify somatic incomplete spikes into uniform amplitudes in mouse cortical pyramidal neurons. PLoS One 5, e11868.
Chorev, E. and Brecht, M. (2012). In vivo dual intra- and extracellular recordings suggest bi-directional coupling between CA1 pyramidal neurons. J. Neurophysiol. 108, 1584–1593.
Colbert, C. and Pan, E. (2002). Ion channel properties underlying axonal action potential initiation in pyramidal neurons. Nat. Neurosci. 5, 533–538.
Coletta, S., Zeraati, R., Nasr, K., Preston-Ferrer, P., and Burgalossi, A. (2018). Interspike interval analysis and spikelets in presubicular head-direction cells. J. Neurophysiol. 120, 564–575.
Connors, B.W. and Kriegstein, A. (1986). Cellular physiology of the turtle visual cortex: distinctive properties of pyramidal and stellate neurons. J. Neurosci. 6, 164–177.
Coombs, J., Eccles, J., and Fatt, P. (1955). The electrical properties of the motoneurone membrane. J. Physiol. 130, 291–325.
Coombs, J., Curtis, D., and Eccles, J. (1957). The interpretation of spike potentials of motoneurones. J. Physiol. 139, 198–231.
Crochet, S., Fuentealba, P., Timofeev, I., and Steriade, M. (2004). Selective amplification of neocortical neuronal output by fast prepotentials in vivo. Cereb. Cortex 14, 1110–1121.
Cruikshank, S., Hopperstad, M., Younger, M., Connors, B., Spray, D., and Srinivas, M. (2004). Potent block of Cx36 and Cx50 gap junction channels by mefloquine. Proc. Natl. Acad. Sci. USA 101, 12364–12369.
Draguhn, A., Traub, R., Schmitz, D., and Jefferys, J. (1998). Electrical coupling underlies high-frequency oscillations in the hippocampus in vitro. Nature 394, 189–192.
Dudek, F., Snow, R., and Taylor, C. (1986). Role of electrical interactions in synchronization of epileptiform bursts. Adv. Neurol. 44, 593–617.
Dugladze, T., Schmitz, D., Whittington, M.A., Vida, I., and Gloveli, T. (2012). Segregation of axonal and somatic activity during fast network oscillations. Science 336, 1458–1461.
English, D.F., Peyrache, A., Stark, E., Roux, L., Vallentin, D., Long, M.A., and Buzsáki, G. (2014). Excitation and inhibition compete to control spiking during hippocampal ripples: intracellular study in behaving mice. J. Neurosci. 34, 16509–16517.
- Export Citation
English, D.F., Peyrache, A., Stark, E., Roux, L., Vallentin, D., Long, M.A., and Buzsáki, G. (2014). Excitation and inhibition compete to control spiking during hippocampal ripples: intracellular study in behaving mice. J. Neurosci.)| false 34, 16509–16517. 10.1523/JNEUROSCI.2600-14.2014 25471587
Epsztein, J., Lee, A., Chorev, E., and Brecht, M. (2010). Impact of spikelets on hippocampal CA1 pyramidal cell activity during spatial exploration. Science 327, 474–477.
Fleidervish, I., Lasser-Ross, N., Gutnick, M., and Ross, W. (2010). Na+ imaging reveals little difference in action potential-evoked Na+ influx between axon and soma. Nat. Neurosci. 13, 852–860.
Fox, J.E., Bikson, M., and Jefferys, J.G. (2004). Tissue resistance changes and the profile of synchronized neuronal activity during ictal events in the low-calcium model of epilepsy. J. Neurophysiol. 92, 181–188.
Fuentealba, P., Crochet, S., Timofeev, I., Bazhenov, M., Sejnowski, T., and Steriade, M. (2004). Experimental evidence and modeling studies support a synchronizing role for electrical coupling in the cat thalamic reticular neurons in vivo. Eur. J. Neurosci. 20, 111–119.
- Export Citation
Fuentealba, P., Crochet, S., Timofeev, I., Bazhenov, M., Sejnowski, T., and Steriade, M. (2004). Experimental evidence and modeling studies support a synchronizing role for electrical coupling in the cat thalamic reticular neurons)| false in vivo. Eur. J. Neurosci. 20, 111–119. 10.1111/j.1460-9568.2004.03462.x 15245484
Galarreta, M. and Hestrin, S. (2001). Electrical synapses between GABA-releasing interneurons. Nat. Rev. Neurosci. 2, 425–433.
Geiger, J.R. and Jonas, P. (2000). Dynamic control of presynaptic Ca2+ inflow by fast-inactivating K+ channels in hippocampal mossy fiber boutons. Neuron 28, 927–939.
Gibson, J.R., Beierlein, M., and Connors, B.W. (2005). Functional properties of electrical synapses between inhibitory interneurons of neocortical layer 4. J. Neurophysiol. 93, 467–480.
Gold, C., Henze, D., Koch, C., and Buzsaki, G. (2006). On the origin of the extracellular action potential waveform: a modeling study. J. Neurophysiol. 95, 3113–3128.
Golding, N. and Spruston, N. (1998). Dendritic sodium spikes are variable triggers of axonal action potentials in hippocampal CA1 pyramidal neurons. Neuron 21, 1189–1200.
González-Nieto, D., Gomez-Hernandez, J., Larrosa, B., Gutierrez, C., Munoz, M., Fasciani, I., O’Brien, J., Zappala, A., Cicirata, F., and Barrio, L. (2008). Regulation of neuronal connexin-36 channels by pH. Proc. Natl. Acad. Sci. USA 105, 17169–17174.
- Export Citation
González-Nieto, D., Gomez-Hernandez, J., Larrosa, B., Gutierrez, C., Munoz, M., Fasciani, I., O’Brien, J., Zappala, A., Cicirata, F., and Barrio, L. (2008). Regulation of neuronal connexin-36 channels by pH. Proc. Natl. Acad. Sci. USA)| false 105, 17169–17174. 10.1073/pnas.0804189105
Grubb, M. and Burrone, J. (2010). Activity-dependent relocation of the axon initial segment fine-tunes neuronal excitability. Nature 465, 1070–1074.
Hamzei-Sichani, F., Kamasawa, N., Janssen, W., Yasumura, T., Davidson, K., Hof, P., Wearne, S., Stewart, M., Young, S., Rash, J.E., and Traub, R. (2007). Gap junctions on hippocampal mossy fiber axons demonstrated by thin-section electron microscopy and freeze–fracture replica immunogold labeling. Proc. Natl. Acad. Sci. USA 104, 12548–12553.
- Export Citation
Hamzei-Sichani, F., Kamasawa, N., Janssen, W., Yasumura, T., Davidson, K., Hof, P., Wearne, S., Stewart, M., Young, S., Rash, J.E., and Traub, R. (2007). Gap junctions on hippocampal mossy fiber axons demonstrated by thin-section electron microscopy and freeze–fracture replica immunogold labeling. Proc. Natl. Acad. Sci. USA)| false 104, 12548–12553. 10.1073/pnas.0705281104
Han, K.-S., Guo, C., Chen, C.H., Witter, L., Osorno, T., and Regehr, W.G. (2018). Ephaptic coupling promotes synchronous firing of cerebellar Purkinje cells. Neuron 100, 564–578.
Holt, G. and Koch, C. (1999). Electrical interactions via the extracellular potential near cell bodies. J. Comp. Neurosci. 6, 169–184.
Holzbecher, A. and Kempter, R. (2018). Interneuronal gap junctions increase synchrony and robustness of hippocampal ripple oscillations. Eur. J. Neurosci. 48, 3446–3465.
Hormuzdi, S.G., Pais, I., LeBeau, F.E., Towers, S.K., Rozov, A., Buhl, E.H., Whittington, M.A., and Monyer, H. (2001). Impaired electrical signaling disrupts gamma frequency oscillations in connexin 36-deficient mice. Neuron 31, 487–495.
- Export Citation
Hormuzdi, S.G., Pais, I., LeBeau, F.E., Towers, S.K., Rozov, A., Buhl, E.H., Whittington, M.A., and Monyer, H. (2001). Impaired electrical signaling disrupts gamma frequency oscillations in connexin 36-deficient mice. Neuron)| false 31, 487–495. 11516404 10.1016/S0896-6273(01)00387-7
Hu, W., Tian, C., Li, T., Yang, M., Hou, H., and Shu, Y. (2009). Distinct contributions of NaV1. 6 and NaV1. 2 in action potential initiation and backpropagation. Nat. Neurosci. 12, 996–1002.
Hughes, S., Blethyn, K., Cope, D., and Crunelli, V. (2002). Properties and origin of spikelets in thalamocortical neurones in vitro. Neurosci. 110, 395–401.
Jarsky, T., Roxin, A., Kath, W.L., and Spruston, N. (2005). Conditional dendritic spike propagation following distal synaptic activation of hippocampal CA1 pyramidal neurons. Nat. Neurosci. 8, 1667–1676.
Jefferys, J. (1995). Nonsynaptic modulation of neuronal activity in the brain: electric currents and extracellular ions. Physiol. Rev. 75, 689–723.
Kandel, E., Spencer, W., and Brinley, F. (1961). Electrophysiology of hippocampal neurons: I. Sequential invasion and synaptic organization. J. Neurophysiol. 24, 225–242.
Kaplan, E. and Shapley, R. (1984). The origin of the S (slow) potential in the mammalian lateral geniculate nucleus. Exp. Brain. Res. 55, 111–116.
Katz, E., Stoler, O., Scheller, A., Khrapunsky, Y., Goebbels, S., Kirchhoff, F., Gutnick, M.J., Wolf, F., and Fleidervish, I.A. (2018). Role of sodium channel subtype in action potential generation by neocortical pyramidal neurons. Proc. Natl. Acad. Sci. USA 115, E7184–E7192.
- Export Citation
Katz, E., Stoler, O., Scheller, A., Khrapunsky, Y., Goebbels, S., Kirchhoff, F., Gutnick, M.J., Wolf, F., and Fleidervish, I.A. (2018). Role of sodium channel subtype in action potential generation by neocortical pyramidal neurons. Proc. Natl. Acad. Sci. USA)| false 115, E7184–E7192. 10.1073/pnas.1720493115
Kole, M., Letzkus, J., and Stuart, G. (2007). Axon initial segment Kv1 channels control axonal action potential waveform and synaptic efficacy. Neuron 55, 633–647.
Konnerth, A., Heinemann, U., and Yaari, Y. (1984). Slow transmission of neural activity in hippocampal area CA1 in absence of active chemical synapses. Nature 307, 69–71.
Kress, G., Dowling, M., Eisenman, L., and Mennerick, S. (2010). Axonal sodium channel distribution shapes the depolarized action potential threshold of dentate granule neurons. Hippocampus 20, 558–571.
Kuba, H., Oichi, Y., and Ohmori, H. (2010). Presynaptic activity regulates Na+ channel distribution at the axon initial segment. Nature 465, 1075–1078.
Larkum, M.E., Watanabe, S., Lasser-Ross, N., Rhodes, P., and Ross, W.N. (2008). Dendritic properties of turtle pyramidal neurons. J. Neurophysiol. 99, 683–694.
Lazarov, E., Dannemeyer, M., Feulner, B., Enderlein, J., Gutnick, M.J., Wolf, F., and Neef, A. (2018). An axon initial segment is required for temporal precision in action potential encoding by neuronal populations. Sci. Adv. 4, eaau8621.
- Export Citation
Lazarov, E., Dannemeyer, M., Feulner, B., Enderlein, J., Gutnick, M.J., Wolf, F., and Neef, A. (2018). An axon initial segment is required for temporal precision in action potential encoding by neuronal populations. Sci. Adv.)| false 4, eaau8621. 10.1126/sciadv.aau8621 30498783
Lezmy, J., Lipinsky, M., Khrapunsky, Y., Patrich, E., Shalom, L., Peretz, A., Fleidervish, I.A., and Attali, B. (2017). M-current inhibition rapidly induces a unique CK2-dependent plasticity of the axon initial segment. Proc. Natl. Acad. Sci. USA 114, E10234–E10243.
- Export Citation
Lezmy, J., Lipinsky, M., Khrapunsky, Y., Patrich, E., Shalom, L., Peretz, A., Fleidervish, I.A., and Attali, B. (2017). M-current inhibition rapidly induces a unique CK2-dependent plasticity of the axon initial segment. Proc. Natl. Acad. Sci. USA)| false 114, E10234–E10243. 10.1073/pnas.1708700114
Li, X., Kamasawa, N., Ciolofan, C., Olson, C.O., Lu, S., Davidson, K.G., Yasumura, T., Shigemoto, R., Rash, J.E., and Nagy, J.I. (2008). Connexin45-containing neuronal gap junctions in rodent retina also contain connexin36 in both apposing hemiplaques, forming bihomotypic gap junctions, with scaffolding contributed by zonula occludens-1. J. Neurosci. 28, 9769–9789.
- Export Citation
Li, X., Kamasawa, N., Ciolofan, C., Olson, C.O., Lu, S., Davidson, K.G., Yasumura, T., Shigemoto, R., Rash, J.E., and Nagy, J.I. (2008). Connexin45-containing neuronal gap junctions in rodent retina also contain connexin36 in both apposing hemiplaques, forming bihomotypic gap junctions, with scaffolding contributed by zonula occludens-1. J. Neurosci.)| false 28, 9769–9789. 10.1523/JNEUROSCI.2137-08.2008 18815262
Llinas, R., Baker, R., and Sotelo, C. (1974). Electrotonic coupling between neurons in cat inferior olive. J. Neurophysiol. 37, 560–571.
Lorincz, A. and Nusser, Z. (2008). Cell-type-dependent molecular composition of the axon initial segment. J. Neurosci. 28, 14329–14340.
Losonczy, A., Makara, J.K., and Magee, J.C. (2008). Compartmentalized dendritic plasticity and input feature storage in neurons. Nature 452, 436–441.
MacVicar, B.A. and Dudek, F.E. (1981). Electrotonic coupling between pyramidal cells: a direct demonstration in rat hippocampal slices. Science 213, 782–785.
Meeks, J. and Mennerick, S. (2007). Action potential initiation and propagation in CA3 pyramidal axons. J. Neurophysiol. 97, 3460–3472.
Mercer, A., Bannister, A., and Thomson, A. (2006). Electrical coupling between pyramidal cells in adult cortical regions. Brain Cell. Biol. 35, 13–27.
Michalikova, M., Remme, M.W.H., and Kempter, R. (2017). Spikelets in pyramidal neurons: action potentials initiated in the axon initial segment that do not activate the soma. PLoS Comp. Biol. 13, e1005237.
Michalikova, M., Remme, M.W.H., and Kempter, R. (2018). Extracellular waveforms reveal an axonal origin of spikelets in pyramidal neurons. J. Neurophysiol. 120, 1484–1495.
Mickus, T., Jung, H.-y., and Spruston, N. (1999). Properties of slow, cumulative sodium channel inactivation in rat hippocampal CA1 pyramidal neurons. Biophys. J. 76, 846–860.
Müller, C., Beck, H., Coulter, D., and Remy, S. (2012). Inhibitory control of linear and supralinear dendritic excitation in CA1 pyramidal neurons. Neuron 75, 851–864.
Nimmrich, V., Maier, N., Schmitz, D., and Draguhn, A. (2005). Induced sharp wave-ripple complexes in the absence of synaptic inhibition in mouse hippocampal slices. J. Physiol. 563, 663–670.
Pais, I., Hormuzdi, S.G., Monyer, H., Traub, R.D., Wood, I.C., Buhl, E.H., Whittington, M.A., and LeBeau, F.E. (2003). Sharp wave-like activity in the hippocampus in vitro in mice lacking the gap junction protein connexin 36. J. Neurophysiol. 89, 2046–2054.
- Export Citation
Pais, I., Hormuzdi, S.G., Monyer, H., Traub, R.D., Wood, I.C., Buhl, E.H., Whittington, M.A., and LeBeau, F.E. (2003). Sharp wave-like activity in the hippocampus in vitro in mice lacking the gap junction protein connexin 36. J. Neurophysiol.)| false 89, 2046–2054. 12686578 10.1152/jn.00549.2002
Palay, S., Sotelo, C., Peters, A., and Orkand, P. (1968). The axon hillock and the initial segment. J. Cell. Biol. 38, 193–201.
Palmer, L. and Stuart, G. (2006). Site of action potential initiation in layer 5 pyramidal neurons. J. Neurosci. 26, 1854–1863.
Remy, S., Csicsvari, J., and Beck, H. (2009). Activity-dependent control of neuronal output by local and global dendritic spike attenuation. Neuron 61, 906–916.
Rouach, N., Segal, M., Koulakoff, A., Giaume, C., and Avignone, E. (2003). Carbenoxolone blockade of neuronal network activity in culture is not mediated by an action on gap junctions. J. Physiol. 553, 729–745.
Royeck, M., Horstmann, M., Remy, S., Reitze, M., Yaari, Y., and Beck, H. (2008). Role of axonal Nav1. 6 sodium channels in action potential initiation of CA1 pyramidal neurons. J. Neurophysiol. 100, 2361–2380.
Rush, A., Dib-Hajj, S., and Waxman, S. (2005). Electrophysiological properties of two axonal sodium channels, Nav1.2 and Nav1.6, expressed in mouse spinal sensory neurones. J. Physiol. 564, 803–815.
Schlingloff, D., Káli, S., Freund, T.F., Hájos, N., and Gulyás, A.I. (2014). Mechanisms of sharp wave initiation and ripple generation. J. Neurosci. 34, 11385–11398.
Schmitz, D., Schuchmann, S., Fisahn, A., Draguhn, A., Buhl, E., Petrasch-Parwez, E., Dermietzel, R., Heinemann, U., and Traub, R. (2001). Axo-axonal coupling: a novel mechanism for ultrafast neuronal communication. Neuron 31, 831–840.
- Export Citation
Schmitz, D., Schuchmann, S., Fisahn, A., Draguhn, A., Buhl, E., Petrasch-Parwez, E., Dermietzel, R., Heinemann, U., and Traub, R. (2001). Axo-axonal coupling: a novel mechanism for ultrafast neuronal communication. Neuron)| false 31, 831–840. 10.1016/S0896-6273(01)00410-X 11567620
Scholl, B., Andoni, S., and Priebe, N.J. (2015). Functional characterization of spikelet activity in the primary visual cortex. J. Physiol. 593, 4979–4994.
Shah, M., Migliore, M., Valencia, I., Cooper, E., and Brown, D. (2008). Functional significance of axonal Kv7 channels in hippocampal pyramidal neurons. Proc. Natl. Acad. Sci. USA 105, 7869–7874.
Sheffield, M., Best, T., Mensh, B., Kath, W., and Spruston, N. (2010). Slow integration leads to persistent action potential firing in distal axons of coupled interneurons. Nat. Neurosci. 14, 200–207.
Snipas, M., Rimkute, L., Kraujalis, T., Maciunas, K., and Bukauskas, F.F. (2017). Functional asymmetry and plasticity of electrical synapses interconnecting neurons through a 36-state model of gap junction channel gating. PLoS Comp. Biol. 13, e1005464.
- Export Citation
Snipas, M., Rimkute, L., Kraujalis, T., Maciunas, K., and Bukauskas, F.F. (2017). Functional asymmetry and plasticity of electrical synapses interconnecting neurons through a 36-state model of gap junction channel gating. PLoS Comp. Biol.)| false 13, e1005464. 10.1371/journal.pcbi.1005464
Spencer, W. and Kandel, E. (1961). Electrophysiology of hippocampal neurons: IV. Fast prepotentials. J. Neurophysiol. 24, 272–285.
Spruston, N., Schiller, Y., Stuart, G., and Sakmann, B. (1995). Activity-dependent action potential invasion and calcium influx into hippocampal CA1 dendrites. Science 268, 297–300.
Stark, E., Roux, L., Eichler, R., Senzai, Y., Royer, S., and Buzsáki, G. (2014). Pyramidal cell-interneuron interactions underlie hippocampal ripple oscillations. Neuron 83, 467–480.
Stuart, G., Schiller, J., and Sakmann, B. (1997). Action potential initiation and propagation in rat neocortical pyramidal neurons. J. Physiol. 505, 617–632.
Su, X., Chen, J.-J., Liu, L.-Y., Huang, Q., Zhang, L.-Z., Li, X.-Y., He, X.-N., Lu, W., Sun, S., Li, H., et al. (2017). Neonatal CX26 removal impairs neocortical development and leads to elevated anxiety. Proc. Natl. Acad. Sci. USA 114, 3228–3233.
- Export Citation
Su, X., Chen, J.-J., Liu, L.-Y., Huang, Q., Zhang, L.-Z., Li, X.-Y., He, X.-N., Lu, W., Sun, S., Li, H., et al. (2017). Neonatal CX26 removal impairs neocortical development and leads to elevated anxiety. Proc. Natl. Acad. Sci. USA)| false 114, 3228–3233. 10.1073/pnas.1613237114
Sun, Q., Srinivas, K.V., Sotayo, A., and Siegelbaum, S.A. (2014). Dendritic Na+ spikes enable cortical input to drive action potential output from hippocampal CA2 pyramidal neurons. eLife 3, e04551.
Tovar, K., Maher, B., and Westbrook, G. (2009). Direct actions of carbenoxolone on synaptic transmission and neuronal membrane properties. J. Neurophysiol. 102, 974–978.
Traub, R., Schmitz, D., Jefferys, J., and Draguhn, A. (1999). High-frequency population oscillations are predicted to occur in hippocampal pyramidal neuronal networks interconnected by axo-axonal gap junctions. Neurosci. 92, 407–426.
Traub, R.D., Kopell, N., Bibbig, A., Buhl, E.H., LeBeau, F.E., and Whittington, M.A. (2001). Gap junctions between interneuron dendrites can enhance synchrony of gamma oscillations in distributed networks. J. Neurosci. 21, 9478–9486.
- Export Citation
Traub, R.D., Kopell, N., Bibbig, A., Buhl, E.H., LeBeau, F.E., and Whittington, M.A. (2001). Gap junctions between interneuron dendrites can enhance synchrony of gamma oscillations in distributed networks. J. Neurosci.)| false 21, 9478–9486. 11717382 10.1523/JNEUROSCI.21-23-09478.2001
Valiante, T., Perez Velazquez, J., Jahromi, S., and Carlen, P. (1995). Coupling potentials in CA1 neurons during calcium-free-induced field burst activity. J. Neurosci. 15, 6946–6956.
Vigmond, E., Perez Velazquez, J., Valiante, T., Bardakjian, B., and Carlen, P. (1997). Mechanisms of electrical coupling between pyramidal cells. J. Neurophysiol. 78, 3107–3116.
Wang, Y., Barakat, A., and Zhou, H. (2010). Electrotonic coupling between pyramidal neurons in the neocortex. PLoS One 5, e10253.
Weiss, S.A. and Faber, D.S. (2010). Field effects in the CNS play functional roles. Front. Neural. Circuit. 4, 15.
Wong, R. and Stewart, M. (1992). Different firing patterns generated in dendrites and somata of CA1 pyramidal neurones in guinea-pig hippocampus. J. Physiol. 457, 675–687.
Xu, J., Kang, N., Jiang, L., Nedergaard, M., and Kang, J. (2005). Activity-dependent long-term potentiation of intrinsic excitability in hippocampal CA1 pyramidal neurons. J. Neurosci. 25, 1750–1760.
Zhang, Y., Perez Velazquez, J., Tian, G., Wu, C., Skinner, F., Carlen, P., and Zhang, L. (1998). Slow oscillations (≤ 1 Hz) mediated by GABAergic interneuronal networks in rat hippocampus. J. Neurosci. 18, 9256–9268.
Zhang, X., Zhang, L., and Carlen, P. (2004). Electrotonic coupling between stratum oriens interneurons in the intact in vitro mouse juvenile hippocampus. J. Physiol. 558, 825–839.