Ca2+ Signals in Astrocytes Facilitate Spread of Epileptiform Activity.

Epileptic seizures are associated with increased astrocytic Ca2+ signaling, but the fine spatiotemporal kinetics of the ictal astrocyte-neuron interplay remains elusive. By using 2-photon imaging of awake head-fixed mice with chronic hippocampal windows we demonstrate that astrocytic Ca2+ signals precede neuronal Ca2+ elevations during the initial bout of kainate-induced seizures. On average, astrocytic Ca2+ elevations preceded neuronal activity in CA1 by about 8 s. In subsequent bouts of epileptic seizures, astrocytes and neurons were activated simultaneously. The initial astrocytic Ca2+ elevation was abolished in mice lacking the type 2 inositol-1,4,5-trisphosphate-receptor (Itpr2-/-). Furthermore, we found that Itpr2-/- mice exhibited 60% less epileptiform activity compared with wild-type mice when assessed by telemetric EEG monitoring. In both genotypes we also demonstrate that spreading depression waves may play a part in seizure termination. Our findings imply a role for astrocytic Ca2+ signals in ictogenesis.

Introduction

Epileptic seizures are characterized by localized or spreading hypersynchronous neuronal activity. The mechanisms underlying this synchronization remain poorly understood. Synaptic and nonsynaptic factors, electrical field transmission as well as astrocytes have been proposed to contribute (Fellin and Haydon 2005; Zhang et al. 2014; Henneberger 2017).

Astrocytes are the main type of glial cells in the CNS, and are about as numerous as neurons (Sherwood et al. 2006; Azevedo et al. 2009). The delicate processes of one single astrocyte could form dynamic contacts with tens of thousands of neurons (Bushong et al. 2002). Furthermore, astrocytes express ion channels, neurotransmitter receptors and transporters and are able to release neuroactive substances. Thus, they are permitted to indirectly modify neuronal excitability by controlling extracellular ion concentration or regulating uptake of neurotransmitters or more directly take part in neuronal signal transduction by active release of signalling substances (Perea et al. 2009; Halassa and Haydon 2010).

The discovery that astrocytes can respond to different physiological and nonphysiological stimuli by intracellular or wave-like intercellular Ca2+ elevations provided the awareness of a new dimension of signal transduction in the brain (Agulhon et al. 2008; Leybaert and Sanderson 2012; Bazargani and Attwell 2016). Such glial Ca2+ transients could possibly trigger release of active substances such as glutamate, d-serine, and ATP (Perea and Araque 2005; Panatier et al. 2011; Perea et al. 2009, 2014).

Along with growing knowledge of astroglial function in the healthy brain, the role of dysfunctional astrocytes in the pathogenesis of neurological disorders, including epilepsy, is now increasingly recognized (Eid et al. 2004; Aronica et al. 2012; Binder et al. 2012; Carmignoto and Haydon 2012; Coulter and Eid 2012; Steinhäuser et al. 2012). Several lines of evidence suggest a role for astrocytes both in epileptogenesis—that is, development of a recurrent seizure phenotype—through malfunctioning reactive astrocytes (Bedner et al. 2015; Steinhäuser et al. 2016; Klein et al. 2018) and ictogenesis—that is, the processes of transition from the interictal state to a seizure—by contributing to neuronal synchronization and spread of epileptic activity (Tian et al. 2005; Gómez-Gonzalo et al. 2010; Henneberger 2017). The interaction between astrocytes and neurons at the very transition from the nonseizing to the seizing state, has been sparsely investigated and provided conflicting results (Tian et al. 2005; Fellin et al. 2006; Gómez-Gonzalo et al. 2010; Baird-Daniel et al. 2017). However, these studies were performed on either brain slices (Fellin et al. 2006; Gómez-Gonzalo et al. 2010) with perturbed connectivity and lack of long-range connections, or in vivo using anesthesia (Baird-Daniel et al. 2017), which has been shown to suppress astrocytic Ca2+ signaling (Thrane et al. 2012).

The objective of the study was to resolve whether astrocytic Ca2+ signals are implicated in the spread of epileptic activity. We set out to assess the spatiotemporal relation between astrocytic and neuronal Ca2+ signals during kainate-induced epileptic seizures in awake mice by doing 2-photon microscopy through chronic window implants to the hippocampus CA1 region. To assess the potential involvement of astrocytic Ca2+ signals in seizures we used knockout mice (Itpr2) lacking the inositol-1,4,5-trisphosphate (IP3) receptor 2 (IP3R2), which mediates Ca2+ release from the endoplasmic reticulum. IP3R2 is the predominant IP3 receptor in astrocytes, and Itpr2 mice exhibit strongly attenuated astroglial Ca2+ signals (Foskett et al. 2007; Srinivasan et al. 2015). We also investigated the seizure susceptibility of the Itpr2 mouse model by EEG telemetry.

Materials and Methods

Animals

Male C57Bl/6J wild-type (WT) (Janvier Labs) and Itpr2−/− (Itpr2; MGI:3640970) (Li et al. 2005) mice of 10–14 weeks of age were used for the experiments. Adequate measures were taken to minimize pain and discomfort. Mice were housed on a 12 h light:12 h dark cycle (lights on at 8 AM), 1–4 mice per cage. All experimental groups contained at least 6 mice. Experiments were carried out in accordance with the guidelines published in the European Communities Council Directive of 24 November 1986 (86/609/EEC). All procedures were approved by the Animal Use and Care Committee of the Institute of Basic Medical Sciences, the Faculty of Medicine at the University of Oslo and the Norwegian Food Safety Authority (project number: FOTS 7128 and 11255).

Virus Production and Transfection

Serotype 2/1 recombinant adeno-associated viruses (rAAV) from plasmid constructs pAAV-GFAP-GCaMP6f (Chen et al. 2013; Enger et al. 2017) and pAAV-SYN-jRGECO1a (Dana et al. 2016), were generated as described (Tang et al. 2009), purified by AVB Sepharose affinity chromatography (Smith et al. 2009) following titration with real-time PCR (rAAV titers about 1.0–6.0 × 1012 viral genomes/mL, TaqMan Assay, Applied Biosystems, Inc.). Approximately 1 week before the chronic hippocampal windows were made, 200 nL of a mixture of the two viruses was injected at coordinates anteroposterior +2.5 mm, lateral +2 mm relative to bregma, at 2 different depths: −900 and −1300 μm relative to the brain surface. Mice used for acute slice experiments were injected bilaterally. The mice were left for 3 more weeks for the fluorescent sensors to be expressed before imaging experiments were performed.

Implantation of Chronic Hippocampus Windows

Anesthesia was induced in a chamber containing 3% isoflurane in room air enriched with 50% pure oxygen and subsequently maintained by nose cone flowing 1–1.5% isoflurane on the same gas mixture. Body temperature was kept at 37 °C by a temperature-controlled heating pad. Buprenorphine 0.15 mg/kg was injected intraperitoneally, and the mice were left for 10 min before surgery started. The field was sterilized, and local analgesia was accomplished by injection of bupivacaine (5 mg/mL). The skull was exposed and cleaned. Groves were cut by scalpel in a checkerboard pattern into the periosteum to strengthen the adhesion of the cyanoacrylate glue that was subsequently applied concomitantly to the attachment of a custom-made titanium head bar. A 2.5 mm craniotomy with center coordinates anteroposterior −2 mm, lateral +2 mm relative to bregma was created as previously described (Dombeck et al. 2010; Kaifosh et al. 2013; Lovett-Barron et al. 2014; Zaremba et al. 2017). In short, a dental drill was used to carefully carve a circular groove in the skull with intermittent air puffs for the removal of debris until approximately 0.1 mm of the bone thickness was left. The bone fragment and the dura was then removed. Subsequently, the cortex was carefully removed with a custom made suction device. Extreme care was taken when approaching the alveus of the hippocampus. The last remnants of the overlying commissural fibers of the corpus callosum were removed with a microspatula. A circular cover glass of 2.5 mm diameter was glued onto a stainless steel cylinder with a similar outer diameter and a height of 1.5 mm. Subsequently, a 200 μm silver wire was glued onto the side of the cylinder, so that it protruded approximately 200 μm below the level of the glass window, to enable local field potential (LFP) measurements. The cylinder was oriented so that the electrode was positioned approximately 2.6 mm posterior to bregma, and 1.3 mm lateral to the midline. Glue was applied to isolate everything but the very tip of the electrode. The cylinder was then centered in the craniotomy, and lowered so that the glass coverslip very slightly depressed the alveus of the hippocampus. The cylinder was subsequently fastened by cyanoacrylate gel glue and dental cement to the skull. An additional silver wire placed epidurally on the contralateral hemisphere served as reference (200 μm diameter, noninsulated). Care was taken to insulate the wires with glue and dental cement. Connectors for the wires were fastened onto the head bar.

Implantation of Telemetric EEG Transmitters

In total, 10 WT and 10 Itpr2 mice were implanted with radio transmitter EEG recording devices (TA10EA-F20; Data Sciences International). After pre-emptive buprenorphine (0.15 mg/kg) mice were anesthetized with isoflurane (same protocol as above). For the implantation of transmitters, a small skin incision was made in the right abdominal region, and a subcutaneous skin pouch was prepared by blunt dissection. A tunnel for the leads was created by careful blunt dissection towards the cranium until reaching the midsagittal incision. Two small craniotomies were made, positioned bilaterally 1.5 mm from the sagittal suture and 1.9 mm posterior to bregma, and 2 stainless steel screws were inserted (screw length 2 mm; thread diameter 0.8 mm). The telemetric implant was placed into the pouch, and the 2 monopolar leads were connected to the screws. The attached leads were covered with conductive glue and dental cement. The exposed cranium was also covered with dental cement and edges were secured by tissue adhesive. Mice were returned to clean cages and kept warm until they recovered from anesthesia and given buprenorphine (0.15 mg/kg, subcutaneously) and meloxicam (2 mg/kg, subcutaneously) postoperatively for 2 days.

Electrophysiology

Acquisition of data was synchronized by custom-written LabVIEW software (National Instruments). The mice were monitored by infrared-sensitive video surveillance. We used a Multiclamp 700B amplifier with headstage CV-7B (Molecular Devices), and the signals were digitized by National Instruments PCIe-6351, X Series Multifunction DAQ (National Instruments). For seizure detection in mice with implanted radio transmitters, the cages were placed on radio receiver plates (RPC-1; Data Sciences International). The signals were recorded in Dataquest A.R.T. 4.00 Gold/Platinum software (Data Sciences International) and exported to MATLAB for analysis. Seizures were elicited by intraperitoneal injection of 10 mg/kg kainate. EEG was recording for 1 h after kainate injected, following 10 min of baseline recording. Artifacts were manually removed from the EEG traces, and a baseline period was defined. The EEG traces were normalized such that the baseline amplitudes were stretched from −1 to 1. Spikes were detected by a custom-made MATLAB script. A spike was defined as a local maximum if the local maximum was the largest local maximum in between 2 subsequent local minima and the valley-to-peak amplitude of the local maximum and a subsequent local minimum was at least 2 normalized units. Any time point of the recording was characterized as being epileptiform or nonepileptiform in a fully automated algorithm when the instantaneous spike rate was above 0.4 Hz on a spike train that was convolved with a normalized Gaussian window of 5 s duration. This threshold was chosen as it performed well across trials in separating baseline activity and obviously pathological EEG activity. For illustrational purposes, spikes were convolved with a normalized Gaussian window with a duration of 60 s for Figure 4b,c. The evaluator was blind to genotype. EEG spectrograms were generated by using the MATLAB implementation of short-time Fourier transform, spectrogram(). EEG power was quantified by the MATLAB function bandpower() in the frequency ranges delta (0–4 Hz), theta (4–8 Hz), alpha (8–13 Hz), beta (13–30 Hz), and gamma (> 30 Hz).

Figure 4.

Seizure characterization by EEG telemetry. (a) EEG radio transmitters were implanted as illustrated. One week following, kainate (10 mg/kg) was administered intraperitoneally, and seizures were recorded by a radio receiver. (b) Traces: Representative EEG traces from the 2 genotypes. Raster plots: spike rates in all mice in both genotypes 60 min after kainate injection (c) Left panel: Mean spike rate over time for all mice in the 2 groups. Right panel: Cumulative spike count in the 2 genotypes. (d) Left panel: Mean spike rate in the 2 groups, P = 0.04. Right panel: Mean percentage of time the EEG is classified as epileptiform (see Materials and Methods), P < 0.01.

In Vitro 2-Photon Microscopy

Acute hippocampal slices were prepared 3–6 weeks after virus transduction. The mice were killed with isoflurane (Baxter) and brains were removed. Transverse slices of 400 μm thickness from the dorsal and middle portion of each hippocampus, were cut with a vibroslicer (Leica VT1200) fitted with a sapphire blade (Ted Pella) in artificial cerebrospinal fluid (ACSF) at 23–25 °C, bubbled with 95% O2 and 5% CO2, containing (in mM): 124 NaCl, 2 KCl, 1.25 KH2PO4, 2 MgSO4, 1 CaCl2, 26 NaHCO3, and 12 glucose (all from Sigma-Aldrich). For all following procedures, the CaCl2 concentration in the ACSF was 2 mM. The slices where then placed in an interface chamber at 32 °C to recover for at least 1 h. One slice was then transferred to a submerged recording chamber that was perfused with ACSF at 4.5 mL/min, 32 ± 1 °C. Tetrodotoxin (TTX; 1 μM; Tocris Bioscience) was added to the ACSF to block voltage-gated sodium channels and thereby block seizure activity. The tissue expressed the same combination of genetically encoded fluorescent indicators as in the in vivo study. A recording electrode (filled with ACSF, 4–8 MΩ) was placed in the CA1 stratum pyramidale to confirm a successful blockage on neuronal action potentials. We used an Axon Multiclamp 700B amplifier, Digidata 1440 digitizer and pClamp10 software (Molecular Devices) for recording and digitalizing LFPs. Similarly, the SYN-jRGECO1a signal was used to ascertain the actions of TTX. GCaMP6f fluorescence was recorded by a 2-photon laser scanning microscope (model Ultima IV; Prairie Technologies) with an XLPLN 25 × WMP 1.05 NA water-immersion objective (Olympus). A Chameleon Vision II (Coherent) laser provided an excitation wavelength of 999 nm. After 5 min of baseline recording, kainate was added to the bath solution for 3.5 min at 3 different concentrations (0.5, 2, or 10 μM). Images of 180 × 180 pixels, representing a field of view of ~180 × 180 μm2 were acquired at a frame rate of approximately 6 Hz.

In Vivo 2-Photon Microscopy

Fluorescence was recorded by 2-photon laser scanning microscopy as previously described (Enger et al. 2017). An excitation wavelength of 999 nm was used. The first imaging session was performed at least 3 weeks after implantation of the chronic imaging window, in all 4 weeks after the virus injection. By that time the tissue robustly expressed fluorescent indicators in both neurons and astrocytes. There were no obvious changes to tissue morphology and astrocytes did not exhibit reactive morphological changes. Mice were then trained for 2–3 days with handling and getting used to head fixation on the spherical treadmill before data collection commenced. Seizures were elicited by injection of 30 mg/kg kainate intraperitoneally. During imaging experiments, mice that exhibited convulsive seizures according to a Racine seizure score of 5 or running seizures were sacrificed. GCaMP6f or jRGECO1a fluorescence was captured in images of 300 × 300 pixels of approximately 170 × 170 μm2 areas in the transition zone between stratum pyramidale and stratum oriens of CA1 of the hippocampus (approximately 200 μm below the hippocampal surface) with frame rates of approximately 50 Hz.

Image Analysis

Imaging data were corrected for motion artifacts using the NoRMCorre movement correction software (Pnevmatikakis and Giovannucci 2017). Image segmentations and analyses were then performed with custom-written MATLAB programs. Regions of interests (ROIs) defining astrocytic compartments were manually drawn over somata, processes, and endfeet of cells with typical astrocytic morphology in the GCaMP6f signal. Similarly, neuronal somata were segmented and signals were extracted from both channels. The relative change in mean fluorescence (ΔF/F0) over time was calculated for each region of interest and subsequently analyzed by custom-written MATLAB scripts. The ΔF/F0 signal was filtered to remove noise with a moving average filter of 0.75 s duration. Subsequently, the built-in MATLAB function findpeaks() was applied to detect events (inspired by Barrett et al. 2018). A threshold of 0.5 and prominence height of 0.5 was used for the findpeaks() algorithm. Epileptic bouts were defined by synchronous elevations of the neuronal Ca2+ signals, where more than 80% of neuronal ROIs exhibited increased fluorescence simultaneously. Interictal astrocytic Ca2+ elevations were defined as astrocytic Ca2+ events (detected with same algorithm as above) that occurred outside the time points defined as epileptic. Additionally, an unbiased description of fluorescent events was performed by extracting signals from an evenly spaced grid of ROIs of 15 × 15 areas. This approach allowed us to demonstrate if regions with no clear cellular structures that were not segmented manually, exhibited altered Ca2+ kinetics. We used a threshold of 10% of max ΔF/F0 to define the time lag between onset of astrocytic and neuronal Ca2+ increase. For the assessment of astrocyte–neuron lag using manually drawn ROIs, the time point of fluorescent increase in a given astrocyte was compared with the mean of the time points of fluorescent increase in the 3 closest neurons. Imaging data from acute brain slices were analyzed with unbiased grid ROIs as described above. To make raster plots of Ca2+ events before, during and after kainate application in slices, Ca2+ events were detected as described above, and the resulting “spike trains” were convolved with a Gaussian window of 30 s and sigma of 10 s. Mean event rate plots were calculated per slice and plotted (Supplementary Fig. S1).

Statistical Analysis

Statistical analyses were performed using generalized linear mixed effects model statistics in MATLAB. This method was chosen because of the hierarchical study design with observations grouped by mouse identity and genotype, and that such models take into account the dependency between observations by including nested variance terms. We set genotype as the predictor variable and included a random intercept for mouse identity. The gamma distribution was used for non-negative, nonzero continuous variables (signal amplitudes, durations, and area under the curve (AUC)) as this gave the best approximation of the data. For astrocyte–neuron time lags, a normal distribution was presumed. Similarly, a Poisson distribution was used for spike frequency data. All data are given as estimated fixed effects by the mixed effects model with corresponding standard errors and P-values. Model fit was evaluated by Akaike information criterion and Bayesian information criterion and the MATLAB function compare() was used to compare different fits. Spike rate and seizure rate from telemetric EEG data was compared with a 2-sample students t-test as these data were nonhierarchical (one observation per animal) and appeared to be normally distributed upon inspection. An alpha-level of 0.05 was used to determine significance. Group sizes were chosen based on typical group sizes in the literature that should be able to reveal biologically significant differences.

Results

Strong Ca2+ Fluorescence in Astrocytes and Neurons During Bouts of Seizures

The first bout of epileptiform activity emerged in the microscope’s field-of-view approximately 15 min after kainate injection. Bouts of seizures were defined as times where more than 80% of neuronal ROIs exhibited elevated Ca2+ signals. We were able to discriminate neuronal (SYN-jRGECO1a) and astrocytic (GFAP-GCaMP6f) fluorescent signals by a combination of color and morphology as described previously (Enger et al. 2017). Prominent fluorescent signals were detected in both astrocytes and neurons in relation to ictal onset (max ∆F/F0 was 1.5 ± 0.1/0.1 and 1.9 ± 0.2/0.2 in neuronal and astrocytic somata, respectively; Figs 1c and 3a,b; Tables 1 and 2). Bouts of seizures lasted approximately 80 s, whereas astrocytic and neuronal Ca2+ transients during seizures lasted roughly 50 s (Figs 1c and 3a,b; Tables 1 and 2). The frequency of epileptic seizures were 0.20 ± 0.06/0.09 bouts/min and 0.11 ± 0.04/0.05 bouts/min in WT and Itpr2 mice, respectively (P = 0.15, see Fig. 3a). During such bouts of seizures, astrocytic Ca2+ event frequency and amplitude were increased and decreased, respectively, in astrocytic processes compared with somata (see Fig. 3b and Table 2). Even though epileptiform activity in the LFP signal was present within a variable period of time of neuronal fluorescence increases, the electrophysiological signals did not always concur with neuronal fluorescence. The reason for this is likely that the tip of the electrode was positioned some distance away (1–2 mm) from the field-of-view and because the low-resistance electrodes we used can detect signals over large distances when neuronal activity is highly synchronized (Lindén et al. 2011). The placement of a chronic LFP electrode within the field-of-view was not possible with the current hippocampal window preparation.

Figure 1.

Simultaneous monitoring of neuronal and astrocytic Ca2+ levels during kainate-induced seizures. (a) Experimental setup and animal monitoring. First, a mixture of rAAV-GFAP-GCaMP6f and rAAV-SYN-jRGECO1a was injected in the right hippocampus. One week later, a 2.5 mm craniotomy was performed and the underlying cortical tissue was carefully removed, exposing the alveus of the hippocampus, followed by insertion of a cylinder with a glass mounted at the bottom and an LFP recording electrode. (b) The mice were left for at least 3 weeks before habituation to head-fixation commenced and the imaging experiment was performed. An infrared camera was used for animal monitoring during the imaging session. (c) Top row: Reference images from the hippocampal CA1 region, with ROIs plotted on the rightmost image: The arrows labeled S, P, and E indicate astrocytic somata, processes and endfeet, respectively; NS signifies neuronal somata. Second row: representative fluorescent traces from the ROIs marked with white arrowheads in the top row. Following rows: Temporal raster plots of fluorescent signals from all ROIs outlined in top row organized by ROI type. Each horizontal line represents fluorescence over time from a single ROI. (d) Similar to (c), but from an Itpr2 mouse. Scale bars: 50 μm.

Figure 3.

Seizure characteristics and Ca2+ dynamics in astrocytes. (a) The rate, duration and amplitude of seizure bouts based on neuronal Ca2+ signalling were similar in the 2 genotypes, whereas the total area under the curve (AUC) of the neuronal Ca2+ signals was reduced in the Itpr2 mice, compared with WT (P = 0.02). (b) Leftmost panel: The rate of astrocytic Ca2+ transients during bouts of seizures. Middle left panel: The amplitudes of astrocytic Ca2+ events during bouts of seizures. Middle right panel: The duration of astrocytic Ca2+ events during bouts of seizures. Rightmost panel: The AUC of astrocytic Ca2+ events during bouts of seizures. (c) Same as (b) but for interictal astrocytic Ca2+ events. See Tables 1 and 2 for group numbers. In (b) and (c), S, P, and E indicate astrocytic somata, processes, and endfeet, respectively.

Table 1

Neuronal Ca2+ dynamics.

	WT	Itpr2 −/−
Ca2+ signal frequency (events/min/ROI)	0.3 ± 0.04/0.04	0.2 ± 0.04/0.05
n (Events, time, mice)	9520, 5 h 46 m,12	5420, 5 h 13 m, 6
Duration (s)	55.6 ± 7.0/10	45.4 ± 7.0/10
n (Signals, ROIs, mice)	7250, 3690, 12	4360, 2300, 6
Amplitude (∆F/F0)	1.5 ± 0.1/0.1	1.2 ± 0.1/0.1
n (Signals, ROIs, mice)	7240,3680,12	4520, 2300, 6
AUC (A.U.)	100.9 ± 10/20	62.6 ± 8.0/10
n (Signals, ROIs, mice)	7300, 3680, 12	4490, 2400, 6

n = numbers in each group; ROI = region-of-interest; AUC = area under the curve; A.U. = arbitrary units.

Table 2

Astroglial Ca2+ dynamics.

	Seizure		Interictal
	WT	Itpr2 −/−	WT	Itpr2 −/−
Ca2+ signal frequency (events/min/ROI)
Astrocyte somata	0.3 ± 0.03/0.04	0.1 ± 0.02/0.02	0.2 ± 0.04/0.04	0.2 ± 0.03/0.04
n (Events, time, mice)	887, 5 h 42 m, 12	305, 5 h 4 m, 6	639, 5 h 42 m, 12	492, 5 h 4 m, 6
Astrocyte processes	0.4 ± 0.05/0.05	0.2 ± 0.03/0.03	0.3 ± 0.04/0.05	0.2 ± 0.04/0.05
n (Events, time, mice)	2440, 5 h 42 m, 12	722, 5 h 4 m, 6	1420, 5 h 42 m, 12	770, 5 h 4 m, 6
Astrocyte endfeet	0.3 ± 0.04/0.04	0.1 ± 0.03/0.03	0.2 ± 0.04/0.04	0.1 ± 0.03/0.04
n (Events, time, mice)	453, 5 h 42 m, 11	65, 5 h 4 m, 4	309, 5 h 42 m, 11	47, 5 h 4 m, 4
Amplitude (∆F/F0)
Astrocyte somata	1.9 ± 0.2/0.2	1.1 ± 0.09/0.1	1.2 ± 0.06/0.07	0.8 ± 0.05/0.06
n (Signals, ROIs, mice)	460, 460, 12	269, 270, 6	646, 646, 12	141, 140, 5
Astrocyte processes	1.8 ± 0.2/0.2	1.0 ± 0.08/0.09	1.1 ± 0.06/0.07	0.8 ± 0.05/0.05
n (Signals, ROIs, mice)	1180, 1180, 12	642, 640, 6	1640, 1640, 12	400, 400, 5
Astrocyte endfeet	1.8 ± 0.2/0.2	0.9 ± 0.08/0.09	1.1 ± 0.06/0.07	0.8 ± 0.1/0.1
n (Signals, ROIs, mice)	233,233,11	57, 57, 4	304, 304, 11	15, 15, 3
Duration (s)
Astrocyte somata	55.3 ± 6.0/7.0	41.1 ± 6.0/8.0	6.0 ± 0.9/1.0	3.8 ± 0.6/0.9
n (Signals, ROIs, mice)	454, 454, 12	286, 290, 6	339, 339, 12	123, 120, 5
Astrocyte processes	56.5 ± 6.0/8.0	48.4 ± 8.0/10	5.6 ± 0.8/1.0	4.4 ± 0.7/1.0
n (Signals, ROIs, mice)	1180, 1180, 12	667, 670, 6	1030, 1030, 12	349, 350, 5
Astrocyte endfeet	57.8 ± 6.0/8.0	57.7 ± 20/40	7.1 ± 1.0/2.0	2.4 ± 0.6/1.0
n (Signals, ROIs, mice)	238, 238, 11	62, 62, 4	205, 205, 11	13, 13, 3
AUC (A.U.)
Astrocyte somata	72.0 ± 10/20	35.3 ± 5.0/6.0	16.6 ± 3.0/6.0	7.7 ± 1.0/2.0
n (Signals, ROIs, mice)	758, 758, 12	344, 340, 6	911, 911, 12	290, 290, 6
Astrocyte processes	72.4 ± 10/20	34.8 ± 4.0/6.0	15.7 ± 3.0/5.0	5.2 ± 0.6/0.8
n (Signals, ROIs, mice)	1880, 1880, 12	744, 740, 6	2360, 2360, 12	628, 630, 6
Astrocyte endfeet	72.9 ± 10/20	31.9 ± 4.0/5.0	16.6 ± 3.0/6.0	9.4 ± 2.0/4.0
n (Signals, ROIs, mice)	351, 351, 11	66, 66, 4	422, 422, 11	47, 47, 4

n = numbers in each group; ROI = region-of-interest; AUC = area under the curve; A.U. = arbitrary units.

Astrocytic Ca2+ responses were strongly diminished in the Itpr2 mice, underscoring that IP3-mediated Ca2+ release from internal stores plays an important role in astrocytic Ca2+ dynamics during seizures. The fluorescent amplitudes during epileptic seizures in all glial ROI subtypes—somata, processes, and endfeet—were reduced by ~50% in the Itpr2 mice (Fig. 3b, P < 0.01 for all comparisons). Similarly, the rate of Ca2+ transients was diminished (P < 0.01 for all comparisons). There was no significant reduction in duration and amplitude of neuronal Ca2+ responses in the Itpr2 mice. However, the total AUC of the neuronal Ca2+ signal during seizures was reduced in the Itpr2 mice, likely reflecting a less pronounced seizure burden (101 ± 10/20 arbitrary units vs. 63 ± 8/10 arbitrary units, P = 0.03, Table 1).

Astrocytic Ca2+ Signals Precede Local Neuronal Ca2+ Activation at the Onset of Kainate-Induced Seizures

Surprisingly, the first cells to be activated locally in the field-of-view were always astrocytes. On average 8.4 ± 1.7 s after the astrocytic activation, fluorescence started to ramp up in neurons (Fig. 2a). Such preactivation of astrocytes was absent in the Itpr2 mice (P < 0.01 and P = 0.3 compared with 0 s time lag, for WT and Itpr2, respectively; Fig. 2a). The astrocytic signals appeared in a synchronized fashion with no obvious directionality (see Fig. 1c). Hence, it is unlikely that the observed Ca2+ elevation was a result of a Ca2+ wave spreading through the astrocyte syncytium. When manually drawing ROIs based on morphology, only a small portion of the total field-of-view is segmented. To assess whether smaller structures not readily distinguished by visual inspection displayed another fluorescent pattern than what we demonstrated above, we segmented the field-of-view into a 15 × 15 squares grid pattern. The resultant, evenly spaced grid of ROIs was covering the full field-of-view, and the ROIs were small enough to pick up activity in minor cellular subcompartments. In line with the analysis of manually segmented ROIs we found a clear preactivation of astrocytes compared with neurons, and no consistent pattern of synchronous or asynchronous activity in the neuronal channel preceding the astrocytic activation. Similar to above, the astrocytic preactivation lasted 8.7 ± 1.7 s in WT mice and was absent in the Itpr2 mice (P < 0.01 and P = 0.43 compared with 0 s time lag, for WT and Itpr2, respectively; Fig. 2b).

Figure 2.

Astrocyte–neuron time lag and SD. (a) The GFAP-GCaMP6f fluorescence signifying astrocytic Ca2+ levels rose several seconds before fluorescence increased in the neurons. When using manually drawn ROIs, signals in astrocytic somata in WT mice preceded nearby neuronal somata by 8.4 ± 1.7 s. In Itpr2 mice, the astrocyte–neuron lag was 2.3 ± 2.8 s. Signal start in the 2 channels was defined as the time point where fluorescence reached 10% of max ΔF/F0. NS = neuronal soma; S = astrocytic soma. Scale bar: 10 μm. (b) Since manually drawn ROIs only segment parts of the total field-of-view, we opted for an automatic approach that segmented the field-of-view into a 15 × 15 grid pattern. The resultant evenly spaced ROIs were tentatively small enough to register low amplitude signals in small subcellular compartments. When analyzing these signals, the astrocytic GFAP-GCaMP6f signal preceded the neuronal SYN-jRGECO1a signal by 8.7 ± 1.7 s in WT. In Itpr2 mice the astrocyte–neuron lag was 1.8 ± 2.9 s. (c) In all experiments, the first bout of epileptic activity was terminated by a fluorescent wave traveling through the field-of-view, whose speed and fluorescent waveform was similar to SD events. (d) Within 1–2 min of the fluorescent wave passing through the field of view, a characteristic DC shift was detected on the local field potential electrode. (e) The propagation speeds for the fluorescent waves were 93 ± 9 μm/s and 125 ± 13 μm/s for WT and Itpr2 mice, respectively, P = 0.049. Scale bar: 50 μm.

Notably, it was only during the first emergence of epileptiform activity the astrocytic Ca2+ signals preceded those of neurons. At later bouts of local epileptiform activity, astrocytes were activated concomitantly to neuronal signals or with varying time delays (astrocyte–neuron time lags were −4.1 ± 2.2 s and −3.1 ± 3.4 s in WT and Itpr2 mice, respectively: P = 0.76 for comparisons between the 2 genotypes and P = 0.06/0.23, respectively, for WT and Itpr2 mice compared with 0 s astrocyte–neuron time delay).

It seems unlikely that the initial preactivation could be due to direct activation of kainic acid receptors (KAR) on astrocytes, as there is no convincing evidence of expression of such receptors in bona fide astrocytes (Jabs et al. 1994; Vargas et al. 2013; Carta et al. 2014). To confirm the lack of functional expression of KARs on astrocytes, we performed a set of control experiments in acute brain slices expressing the same combination of fluorescent indicators as in the in vivo experiments, using TTX to block neuronal epileptiform activity. LFP recordings and concomitant expression of Ca2+ indicators in neurons confirmed a successful blockage of neurons. Since kainate to a very little degree passes the blood–brain barrier (Gynther et al. 2015), only a small fraction of kainate reaches the brain interstitium following intraperitoneal administration. Typical doses that are sufficient to elicit epileptiform activity in slices are as low as, or even lower than, 500 nM (Ben-Ari and Cossart 2000). Hence, we performed our control experiments with 500 nM kainate concentration (n = 10 slices, 4 mice) concomitant to 2-photon microscopy of astrocytic responses. There was no increase in astrocyte Ca2+ event frequency or total AUC following kainate exposure (Supplementary Fig. S1). A subset of experiments were also carried out with 2 μM kainate concentration (n = 4 slices, 2 mice) and 10 μM kainate concentration (n = 5 slices, 2 mice), similarly demonstrating no increase in astrocyte Ca2+ signaling upon kainate application. Hence, a direct or in-direct activation of astrocytes through activity proximally in the mossy fiber-CA3-CA1 hippocampal trisynaptic circuit or other mechanisms are more likely to be the cause of the observed astrocytic preactivation.

Termination of the First Bout of Seizure

In all experiments, the first round of epileptiform activity was terminated by a prominent increase in the neuronal Ca2+ signal traveling as a wave through the field-of-view with a speed of 93 ± 9 μm/s (Fig. 2c,e). The propagation speeds of these waves were significantly faster in the Itpr2 mice (125 ± 13 μm/s, P = 0.049). Both the speed and the amplitude of the signal in the neuronal channel suggested that the observed wave phenomenon was a spreading depression (SD) event, and the faster propagation speed in the Itpr2 is consistent with previously published data (Enger et al. 2017). There was a further increase in astrocytic Ca2+ fluorescence accompanying the SD events, typically following the neuronal fluorescent changes, but with a time delay of about 1 s, similar to what has previously been demonstrated in a pure SD model (Enger et al. 2017).

Although the LFP recording electrodes were not in immediate vicinity of the imaging field-of-view and the LFP signal was high-pass filtered (0.1 Hz), DC-shifts associated with spreading depolarizations were registered in a subset of experiments within a couple of minutes of the fluorescent waves. The wave phenomenon was followed by a period of quiescence in both recording channels. Within a few minutes, epileptiform activity re-emerged.

Interictal Ca2+ Activity in Astrocytes

Astrocytes also exhibited interictal “spontaneous” Ca2+ signals at times where no neuronal Ca2+ signals were detectable. These appeared at a rate of 0.3, 0.4 and 0.3 spikes per ROI per minute in somata, processes and endfeet, respectively (Fig. 3c and Table 2). They were of lower amplitude (P < 0.001 for all comparisons, Table 2) and shorter duration (P < 0.001 for all comparisons; Table 2) than during epileptiform activity. Astrocytic processes exhibited higher Ca2+ spike rates than somata (P = 0.02). Furthermore, there was a tendency towards a lower Ca2+ signal amplitude in processes compared with somata (P = 0.05). Both the signal amplitude and AUC of the astrocytic Ca2+ signals were reduced in the Itpr2 mice (P < 0.05 for all comparisons, except AUC for the endfoot subcompartment where P = 0.2).

Seizure Characterization by Telemetric EEG Monitoring

In the Ca2+ imaging trials we observed a reduction in neuronal Ca2+ signal AUC in the Itpr2 mice (see above). However, when doing 2-photon imaging in the hippocampus, we were not able to have a continuous monitoring of the mice for extended periods of time after kainate administration. Furthermore, the kainate dose used during 2-photon microscopy (30 mg/kg) may have been too high to clearly reveal differences between the 2 genotypes. Consequently, to assess whether seizure propensity differed between the 2 genotypes, we lowered the kainate dose and took advantage of chronically implanted EEG telemetry (Fig. 4a).

Both WT and Itpr2 mice robustly developed seizures also with a low to moderate dose of kainate (10 mg/kg intraperitoneal). The seizure load was, however, markedly different in the 2 genotypes. Consistently, the Itpr2 mice developed less epileptiform activity. In the 60 min recorded after kainate injection, WT mice had electrographic seizures on average 51 ± 6% of the time, compared with 19 ± 5% of the time in the Itpr2 mice (P < 0.01; Fig. 4b–d). The spike rates were also markedly different in the 2 genotypes (75 ± 18 spikes/min vs. 30 ± 11 spikes/min, for WT and Itpr2, respectively, P = 0.04; Fig. 4d). Spectral analyses of the EEG signals revealed lower power in the beta and gamma frequency bands in the Itpr2−/− mice (see Supplementary Fig. S2). For EEG spectrograms, see Supplementary Figure S1.

Discussion

Here, we used 2-photon microscopy and genetically encoded Ca2+ indicators to reveal Ca2+ signals in hippocampal astrocytes and neurons of awake mice during kainate-induced seizures. Strikingly, prominent astrocytic Ca2+ transients preceded local hypersynchronous neuronal activity during the initial bout of seizure activity. This phenomenon was abolished in Itpr2 mice, indicating that the early astrocytic Ca2+ transients rely on IP3R2 mediated Ca2+ release from the endoplasmic reticulum. Furthermore, we report that Itpr2 mice display less epileptic activity than WT mice, suggesting a proconvulsant role of astrocytic Ca2+ elevations. We also demonstrated that SD and epileptic activity coexist in both genotypes, and observed that SD reliably terminates local neuronal seizure activity.

The first cells to be activated locally in the field-of-view following intraperitoneal administration of kainate were always astrocytes. Their fluorescence increased several seconds before detectable synchronous activation of local neurons. This begs the question—what triggers the initial astrocytic activation?

Both the lack of convincing evidence of expression of KARs in bona fide astrocytes and our own slice experiments makes it highly unlikely that the observed preactivation is due to a direct effect of kainate on the astrocytes (Jabs et al. 1994; Vargas et al. 2013; Carta et al. 2014). However, the hippocampus displays a high density of KARs, and both light- and electron microscopy studies have demonstrated that KAR labeling primarily corresponds to presynaptic and postsynaptic mossy fiber synapses in particular in the CA3 region (Darstein et al. 2003; Ruiz 2005). Consequently, CA3 is thought to be the part of the hippocampus that is the most susceptible to low concentrations of kainate (Monaghan and Cotman 1982; Carta et al. 2014). As our field-of-view was limited to a circumscribed part of the CA1 region, it is highly improbable that we were able to directly detect the starting point of KAR mediated activation of the local hippocampal circuitry. Hence, it is likely that the observed initial astrocyte activation was directly or indirectly elicited by neuronal activity proximally in the mossy fiber-CA3-CA1 hippocampal trisynaptic circuit, although we cannot rule out direct ionotropic and metabotropic effects of kainate on the CA1 pyramidal neurons in the field-of-view (Melyan et al. 2002; Ruiz 2005; Carta et al. 2014). In line with this, it has been shown in numerous studies that astrocytic Ca2+ signals can be elicited by glutamatergic signaling (Porter and McCarthy 1996; Perea and Araque 2005; Schummers et al. 2008; Nimmerjahn et al. 2009).

Studies have demonstrated high activity in inhibitory neurons preceding local recruitment of excitatory neurons in seizures (Avoli and de Curtis 2011; Truccolo et al. 2011; Grasse et al. 2013; Toyoda et al. 2015; Khoshkhoo et al. 2017; Librizzi et al. 2017). Hence, the astrocytic preactivation could be mediated by activity in inhibitory neurons. Indeed, astrocytes have been shown to express both ionotropic and metabotropic GABA receptors (Nedergaard and Verkhratsky 2012; Parpura and Verkhratsky 2013). However, we should have been able to detect activity in interneurons with our experimental setup, as the human SYNAPSIN-1 promoter is known to be expressed in both excitatory and inhibitory neurons (Nathanson et al. 2009). Even though our imaging plane was largely dominated by the excitatory neurons of stratum pyramidale, imaging planes were always placed obliquely to be able to pick up activity in stratum oriens—where we would expect to find more interneuron somata. Still, we found no evidence of neuronal activity concomitant to the astrocytic preactivation in any neuronal compartments in the field-of-view.

Long-range cholinergic (Takata et al. 2011; Chen et al. 2012) or noradrenergic (Bekar et al. 2008; Ding et al. 2013; Paukert et al. 2014) neuromodulatory projections have been shown to mediate coordinated Ca2+ signaling in astrocytes in the cortex. Most likely, hippocampal astrocytes could be activated in a similar fashion. Thus, also long-range neuromodulatory projections could mediate the astrocytic preactivation (Porter and McCarthy 1996; Perea and Araque 2005).

Given our findings, the concept of a role of astrocytes in the recruitment of neurons to seizure activity is tempting. Several known intrinsic astrocyte–neuron interactions can provide the underlying mechanisms, because of their ability to create excitatory feedback loops (Gómez-Gonzalo et al. 2010; Henneberger 2017). Astrocyte-mediated glutamate release and subsequent NMDA receptor stimulation has attracted most attention (Parpura et al. 1994; Tian et al. 2005; Crunelli and Carmignoto 2013), but other neuroactive molecules may also provoke synchronization of local neuronal activity (reviewed in (Perea et al. 2009)). Our observation that Itpr2 seemingly have differential effects on SD (higher propagation speed) and seizure activity (lower seizure burden) is difficult to explain, but may suggest another action of astrocytic Ca2+ signals in the context of ictogenesis than promoting gliotransmitter release. If one considers SD as a potential mechanism for curbing seizure activity, and that this mechanism may partly explain the lower total amount of seizure activity in the Itpr2 mouse model, impaired astrocytic K+ uptake in the knockout mice could be a mechanism linking the 2 observations. It has been shown that astrocytic Ca2+ signals may stimulate astrocytic Na+/K+ ATPase activity (Wang et al. 2012), effectively lowering extracellular K+ concentrations. Hence, the lack of astrocytic Ca2+ signals could in theory lead to higher extracellular K+ levels promoting seizure termination by SD. These hypotheses should be investigated in future studies.

Our findings are supported by results from Nedergaard and coworkers, who observed paroxysmal depolarization shifts in neurons as a result of astrocytic Ca2+ elevations, as well as stereotypical astrocytic Ca2+ signals during seizure activity (Tian et al. 2005). However, recently published data from an in vivo rat model for focal neocortical seizures (Baird-Daniel et al. 2017) conflict with our results. Baird-Daniel et al. reported that seizures were associated with a glial Ca2+ wave that was “markedly delayed after both neuronal and hemodynamic onset” and that this astrocytic Ca2+ elevation was of minor—if any—importance in ictogenesis. The discrepancies between their and our findings may rely on differences in experimental setups, including choice of species, chemoconvulsant and type of Ca2+ indicator. Notably, Baird-Daniel et al. used less sensitive bulk-loaded synthetic Ca2+ dyes, as discussed below. Also, astrocyte heterogeneity and regional differences in network excitability may play a role. It is well established that hippocampal and cortical astrocytes differ in morphology and function, including neurotransmitter receptor expression and Ca2+ signaling (Oberheim et al. 2012). Distinct roles of hippocampal astrocytes, and particular properties in their Ca2+ mediated cell communication may explain why the hippocampus is especially seizure prone (Harris-White et al. 1998). Moreover, the study of Baird-Daniel et al. may be confounded by the use of anesthetics, as these markedly suppress astrocytic Ca2+ signaling (Thrane et al. 2012). Our in vivo experiments were conducted without the use of anesthesia.

While local hippocampal astrocytes were activated seconds before neurons during the first seizure, they were typically activated concomitantly or at varying time delays compared with local neurons in the following ictal episodes. Consequently, the tissue must have undergone pathophysiological and/or morphological changes as a direct result of the initial insult. A multitude of changes entailing time scales from milliseconds to minutes may occur upon the first ictal event that could perturb intrinsic interactions between astrocytes and neurons, and quickly increase network excitability (Henneberger 2017).

The first round of epileptiform activity was always terminated by a slowly propagating wave of high amplitude Ca2+ elevation in both neurons and astrocytes. Also, some subsequent bouts of epilepsy ended in a similar fashion. These waves matched the characteristics of SD waves as previously reported (Enger et al. 2015, 2017; Khoshkhoo et al. 2017), including SD events in association with seizure activity observed in electrophysiological studies (Fabricius et al. 2008). Although the LFP measurement electrodes could not be placed directly in the field-of-view, characteristic DC-shifts were registered in association with such fluorescent waves. This observation is interesting not the least from a clinical point of view: the pathological phenomena of seizures and SD have been recognized to share essential pathophysiological features (Rogawski 2008; Dreier et al. 2012; Wei et al. 2014; Mantegazza and Cestèle 2018). The hallmark of both migraine and epilepsy is a paroxysmal dysfunction of cellular/network excitability and, furthermore, both conditions are highly co-morbid and respond to antiepileptic drugs (Rogawski and Löscher 2004; Keezer et al. 2015).

Several mechanisms on different size scales are proposed to be involved in seizure termination, ranging from the single cell to local networks and brain-wide circuits (Lado and Moshé 2008; Kramer et al. 2012). Still, how seizures terminate remains one of the most important unanswered questions in epileptology (Lado and Moshé 2008). Our experiments provide the first in vivo visualization of concomitant occurrence of seizure activity and SD in the hippocampus, and perhaps more importantly, demonstrate that SD reliably terminates local neuronal activity. In SD models, it is well known that SD silences evoked synaptic activity for several minutes (for review: (Lauritzen et al. 2011; Dreier et al. 2012)). Therefore, it is not surprising that SD also could depress epileptiform activity, and potentially contribute to seizure termination. Understanding the critical step towards the return to the interictal state could identify novel targets for therapeutic action. However, whether SD is an epiphenomenon of ictal activity or a compensatory mechanism to curb seizure activity remains to be determined.

Traditional bulk-loaded synthetic Ca2+ indicators only delineate the soma and largest processes of the astrocyte (Reeves et al. 2011; Leybaert and Sanderson 2012). However, astrocyte–neuron communication does not necessarily involve Ca2+ signals in the astrocytic soma, but may occur in processes and endfeet (Panatier et al. 2011; Szokol et al. 2015). Improved imaging techniques and the development of genetically encoded Ca2+ indicators now allow us to assess focal and small-scale Ca2+ transients in these subcellular compartments (Kanemaru et al. 2014; Srinivasan et al. 2015). In our study, we used the Ca2+ indicator GCaMP6f, which out-performs synthetic Ca2+ indicators both in terms of signal-to-noise ratio and to which degree they outline astrocytic territories (Srinivasan et al. 2015). Notably, we find higher rates of Ca2+ transients both during seizures and between bouts of seizures in astrocytic processes, highlighting a complexity of astrocytic Ca2+ signaling that would have been lost using bulk-loaded Ca2+ indicators.

Here, for the first time, we demonstrate an attenuated seizure burden in Itpr2 mice after exposure to kainate. The Itpr2 knockout mouse model has been used extensively to study the impact of astrocytic Ca2+ signals, but it is becoming more and more clear that these mice still exhibit astrocytic Ca2+ signals both in physiology (Srinivasan et al. 2015)—and to a larger extent—in pathophysiology (Enger et al. 2017). Notwithstanding, this mouse model lacks one of the main pathways that mediate intracellular Ca2+ elevations in astrocytes, and large synchronized Ca2+ elevations are absent during physiological stimuli in these mice. We found that the astrocytic preactivation observed in WT animals was abolished in the Itpr2 mice. We also showed that there was a strong reduction in astrocytic Ca2+ signaling in these mice, although prominent Ca2+ transients still were present. There was also a lower seizure burden when considering AUC of the neuronal Ca2+ signal. This tendency was confirmed and underscored in a more sensitive essay comprising telemetric EEG monitoring, demonstrating a substantially lower seizure burden in the Itpr2 compared with WT.

IP3 receptors are mediators of second messenger-induced intracellular Ca2+ release and 3 IP3 receptor isoforms are known. IP3R2 is the predominant IP3 receptor in glial cells, and is thought to be the key functional IP3 receptor in astrocytes (Sharp et al. 1999; Foskett et al. 2007). Lack of IP3R2 has been shown to abolish both spontaneous and Gq-linked G-protein coupled receptor mediated increases in hippocampal astrocyte Ca2+ transients (Petravicz et al. 2008). Regardless of the importance of IP3 as second messenger for astrocytic Ca2+ dynamics, mice lacking IP3R2 are overtly normal (Petravicz et al. 2008). Accordingly, several recent studies have questioned the physiological importance of astrocyte Ca2+ signaling, by for instance demonstrating normal synaptic transmission and plasticity in these mice (Agulhon et al. 2010; Nizar et al. 2013; Petravicz et al. 2014). Importantly, recent in vivo state-of-the art imaging techniques with new genetically encoded Ca2+ indicators (GCaMP6f, as used in this study) showed that Ca2+ fluctuations are not markedly altered in astrocyte processes of Itpr2 mice although Ca2+ signals in somata are strongly reduced (Srinivasan et al. 2015). Our data demonstrate a strong reduction of Ca2+ events also in astrocytic subcompartments, highlighting another difference between the seizing or interictal brain state compared with physiologic activation.

Interestingly, the reduction of AUC of the astrocytic Ca2+ signal in Itpr2 mice versus WT mice in endfeet failed to reach statistical significance (P = 0.2). In contrast, both duration and amplitude of these signals are significantly lower. The lack of effect of Itpr2 on the AUC in endfeet could imply that other mechanisms of Ca2+ increase than through IP3-receptors play a relatively more important role in endfeet than in other astrocytic subcompartments. A likely explanation is that endfeet, due to their high expression of aquaporin-4 water channels (Nielsen et al. 1997), are more prone to glutamate- and potassium-induced swelling, and hence swelling-induced Ca2+ signals, than other astrocytic subcompartments. It is also possible that transient receptor potential cation channel subfamily V member 4 (TRPV4), a swelling-sensitive cation channel enriched in endfeet, mediates Ca2+ entry into endfeet during our experimental conditions (Jo et al. 2015; Toft-Bertelsen et al. 2018).

Although the downstream effects of astrocytic Ca2+ elevations remain unclear, it is worth noting that propagation speed of SD was markedly increased in Itpr2 mice. We have previously reported that SD waves triggered by elevated K+ also propagate faster in these knockouts than in WT mice (Enger et al. 2017). It is tempting to ascribe parts of the genotype differences in seizure activity to altered SD kinetics in the knockout mice.

Conclusion

We demonstrate that prominent astroglial Ca2+ activity precedes local neuronal activity during spread of kainate-induced seizures in the intact hippocampus of awake mice. This preactivation of glia is abolished in Itpr2 mice, which exhibit reduced epileptiform activity when compared with WT mice. In all, our data suggest a proconvulsive role of astrocytic Ca2+ elevations. The contribution of astrocytic Ca2+ signals are probably modulatory rather than an integral part of seizure propagation as Itpr2 mice with strongly attenuated Ca2+ signals in astrocytes still develop seizures. Nonetheless, this modulatory activity may leave astrocytic Ca2+ signaling a promising target for therapeutic intervention.

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