Introduction

Developmental and Epileptic Encephalopathies (DEEs) are a devastating group of rare epilepsies and neurodevelopmental disorders (Scheffer, French et al. 2016, Scheffer, Berkovic et al. 2017, Scheffer and Liao 2020) that affect 4 in 10,000 infants per year (Covanis 2012, Ware, Huskins et al. 2019). DEEs are characterized by repeated seizures, severe developmental delay, and are often drug resistant. Febrile seizures, which are more common in young children, can contribute to the progression of disease (Skotte, Fadista et al. 2022). DEEs are lethal when the seizures lead to Sudden Unexpected Death in Epilepsy (SUDEP) (Scheffer and Nabbout 2019, Chilcott, Diaz et al. 2022, Donnan, Schneider et al. 2023). Although not all DEEs have been linked to a genetic basis, variants in ion channels and their auxiliary proteins are among the best-characterized genetic causes for DEEs, and sodium channelopathies have been identified as a top cause (Meisler, Hill et al. 2021).

Epilepsy-associated variants in voltage-gated sodium channels (Na_vs), necessary for action potential initiation, exert gain-of-function effects in excitatory neurons or loss of function effects in inhibitory neurons, leading to an overall pro-excitatory state. Gain-of-function variants in SCN8A coding for the neuronal sodium channel Na_V1.6 (Adam, Feldman et al. 1993, Bunton-Stasyshyn, Wagnon et al. 2019, Meisler 2019, Talwar and Hammer 2021) or SCN2A coding for Na_V1.2 (Kim, Yang et al. 2020, Li, Jancovski et al. 2021) (Miao, Tang et al. 2020) affect excitatory neurons of the forebrain, and lead to network hyperexcitability that drives seizures. In contrast, loss-of-function variants in SCN1A coding for Na_V1.1, the most abundant Na_V expressed in forebrain inhibitory neurons, reduce inhibitory drive to excitatory neurons and thus drive network hyperexcitability as the mechanism for seizures (Vormstein-Schneider, Lin et al. 2020, Ding, Li et al. 2021). Variants in Na_V1.1 underlie the most common genetic subgroup in the prototypical DEE, Dravet Syndrome (Scheffer and Nabbout 2019, Han, Chen et al. 2020, Brunklaus, Pérez-Palma et al. 2022, He, Li et al. 2022). DEEs also result from variants in Na_V auxiliary subunits, such as in the Na_V beta subunit SCN1B (Patino, Claes et al. 2009, Ogiwara, Nakayama et al. 2012, Kim, Dibbens et al. 2013, Ramadan, Patel et al. 2017, Bouza and Isom 2018, Hull, O’Malley et al. 2020) as well as FGF12 (Siekierska, Isrie et al. 2016, Oda, Uchiyama et al. 2019, Saleem, Chencheri et al. 2024) and FGF13 (Puranam, He et al. 2015, Fry, Marra et al. 2021, Velíšková, Marra et al. 2021, Narayanan, Majethia et al. 2022), both fibroblast growth factor homologous factors (FHFs) (Goldfarb 2005).

Here, we focus on FGF13, which is expressed in both excitatory and inhibitory neurons (Puranam, He et al. 2015, Joglekar, Prjibelski et al. 2021). Like other members of the FHF family (FGF11-14), FGF13 is a non-canonical fibroblast growth factor that is not secreted and does not bind to FGF receptors (Schoorlemmer and Goldfarb 2001, Olsen, Garbi et al. 2003). FHFs reside in the cytoplasm where they can bind to the intracellular C-terminus of various Na_Vs and modulate their function (Goldfarb 2005, Pablo, Wang et al. 2016). FGF13 has been shown to be upregulated in the hippocampus of a temporal lobe epilepsy mouse model, whereas knockdown of Fgf13 attenuated hyperexcitability in hippocampal cells (Shen, Yue et al. 2022). Other FGF13 functions, such as the regulation of microtubules (Wu, Yang et al. 2012), control of mitogen-activated protein kinases (Lu, Shi et al. 2015), and effects on neurodevelopment (Nishimoto and Nishida 2007) including development of chandelier cells (Favuzzi, Deogracias et al. 2019) have been ascribed, but less well characterized. Moreover, the full complement of FGF13 functions has yet to be defined, obscuring insight into how FGF13 variants lead to DEEs.

While DEE associated variants in FGF13 are thought to affect Na_V function, this has not been demonstrated in neurons and the contribution of other FGF13 functions has not been investigated, thus preventing an understanding of disease pathology and the development of precision therapies. Lack of mechanistic clarity also arises because DEE associated variants in FGF13 have been proposed to cause gain-of-function effects in excitatory neurons (Fry, Marra et al. 2021) or via an apparently contradictory loss-of-function mechanism in inhibitory neurons (Puranam, He et al. 2015). Further complicating mechanistic understanding, FGF13 can generate multiple isoforms, driven by alternative promoter usage and consequent alternative splicing, with different but overlapping functions (Munoz-Sanjuan, Smallwood et al. 2000, Puranam, He et al. 2015). We recently discovered that alternatively spliced Fgf13 mRNAs exhibit distinct cell type-specific expression in the mouse cortex. In the developing mouse brain excitatory neurons express almost exclusively Fgf13-S while inhibitory neurons express both Fgf13-S and Fgf13-VY, a notable example of differential expression of an alternatively spliced neuronal gene in excitatory vs. inhibitory neurons (Furlanis, Traunmuller et al. 2019, Joglekar, Prjibelski et al. 2021). This cell type-specific alternative splicing pattern is similar to other genes which are implicated in the control of synaptic interactions in the hippocampus (Furlanis, Traunmuller et al. 2019), yet the differential splicing complicates the understanding of current models.

DEE associated variants in FGF13 have been identified in FGF13-S and modeled as causing pro-excitatory Na_V channel dysfunction in excitatory neurons. Conversely, a maternally transmitted chromosomal translocation that disrupts the X-linked FGF13 locus and eliminates FGF13-VY expression while preserving expression of FGF13-S causes a seizure disorder in two brothers (Puranam, He et al. 2015). Thus, how FGF13 variants confer seizure susceptibility is unclear. Finally, whether FGF13 variants even exert their effects through Na_V dysfunction or through alternative mechanisms has not been defined.

We generated a series of conditional knockout mouse lines to probe FGF13 function in excitatory and inhibitory hippocampal neurons and investigated the isoform-specific and cell type mechanisms by which variants in Fgf13 cause DEEs. We define a critical role for FGF13 in interneurons but not excitatory neurons underlying a pro-excitatory state associated with seizures. Moreover, as we observe limited effects on Na_V currents underlying the changes associated with a pro-excitatory state, our data add to growing observations that FGF13 can function independently of Na_Vs.

Methods

Animals

Mice were handled in accordance with the ethical guidelines of the National Institutes of Health Guide for the Care and Use of Laboratory Animals. This study was approved by the Weill Cornell Medical Center Institutional Animal Care and Use Committee. Genetically modified mice were maintained on C57BL6/J background (000664; The Jackson Laboratory, Bar Harbor, ME, USA). All mice were maintained on a standard rodent chow diet (PicoLab Rodent Diet 20; 5053; LabDiet, St. Louis, MO, USA) with a 12-h light/dark cycle. Mice were weaned at post-natal day 21 (P21) and group housed in cages holding between two and five mice. To generate neuron-specific mutant mice, female Fgf13^fl/fl mice (Wang, Tang et al. 2017) were crossed with male Nestin-Cre^+/-(B6.Cg-Tg(Nes-cre)1Kln/J, JAX #003771) to produce male hemizygous knockouts (Nestin^{Fgf13 KO}), female heterozygous mutants (Nestin^{Fgf13 HET}), and wild type littermates. To generate excitatory neuron-targeted mutant mice, female Fgf13^fl/fl mice were crossed with male Emx1-Cre^+/-(B6.129S2-Emx1tm1(cre)Krj/J, #005628) to produce male hemizygous knockouts (Emx1^{Fgf13 KO}), female heterozygous mutants (Emx1^{Fgf13 HET}), and wild type littermates. Female Emx1 knockouts were generated by crossing male hemizygous knockouts (Emx1^{Fgf13 KO}) with female Fgf13^fl/flmice. To generate interneuron-specific mutant mice, male Gad2-Cre^+/-(Gad2tm2(cre)Zjh/J, #010802) were crossed with female Fgf13^fl/flmice to produce male hemizygous knockouts (Gad2^{Fgf13 KO}), female heterozygous mutants (Gad2^{Fgf13 HET}), and wild type littermates. To generate interneuron-GFP reporter mice, male Gad2-Cre^+/+(Gad2tm2(cre)Zjh/J, #010802) were crossed with Cre-dependent Ai6^+/+ mice (B6.Cg-Gt(ROSA)26Sortm6(CAG-ZsGreen1)Hze/J), and the resulting Gad2^GFP (Gad2-Cre^+/-; Ai6^+/-) males were crossed with female Fgf13^fl/fl mice to generate Fgf13 knockout interneuron-GFP reporter mice (Gad2-Cre^+/-; Fgf13^FL/Y; Ai6^+/- or Gad2^{GFP-Fgf13 KO}). To generate medial ganglionic eminence (MGE) derived interneuron-targeted mutant mice, female Fgf13^fl/fl mice were crossed with male Nkx2.1-Cre^+/- (C57BL/6J-Tg(Nkx2-1-cre)2Sand/J, # 008661) to produce male hemizygous knockouts (Nkx2.1^{Fgf13 KO}), female heterozygous mutants (Nkx2.1^{Fgf13 HET}), and wild type littermates.

Hyperthermia induced seizures

Mice at P12 were tested using a modified protocol (Cheah, Yu et al. 2012, Puranam, He et al. 2015). Mouse core body temperature was recorded with a rodent rectal temperature probe placed at a depth of 1 cm and connected to a rodent temperature controller (TCAT-2DF, Physitemp). Behavior was monitored by a video camera (Logitech). Command temperature ± 0.3°C was maintained using an infrared heat lamp positioned directly over the recording chamber (2L glass beaker). Mice were acclimated to the chamber for 5 minutes, and any mice with a lower core body temperature were warmed with the heat lamp up to 36.5°C. For baseline monitoring, temperature was adjusted to an initial set-point of 36.5 °C for 5 minutes. Body temperature was elevated in 0.5 °C increments, for 2 minutes at each increment. Temperature was increased until a seizure or 42.0 °C was reached. At the end of hyperthermia induction, mice were placed on a room temperature surface to recover and monitored for 10 minutes.

Electroencephalogram recording

Animal preparation

Mice (P12) were anesthetized under isoflurane (3.5% induction, 1-2% maintenance), provided pre-surgical analgesia (Meloxicam, 2mg/kg SC; Bupivicaine 0.15 ml under scalp), and head-fixed in a stereotaxic frame (KOPF Instruments) with ear bars and an anesthesia-passing nose cone. A heatpad was placed under the animal and the eyes were protected with ointment (Paralube Vet). Hair was removed with fine scissors and an oval-shaped incision (∼4×6 mm) was made on the scalp to expose the skull. Fine forceps were used to scrape the membrane, remove any remaining hair, and expose bregma and skull sutures. The hippocampal EEG site was located at -2.5 mm AP, 1.5 mm ML, -1.25 mm DV. A dental drill was then used to open small craniotomies at the (AP, ML) sites for EEG contacts with a 0.5 mm bur (Meisinger). Reference and ground contact craniotomies were made on the contralateral skull. The EEG recording system (Pinnacle Technology Inc) was attached to headmounts (Pinnacle product #8201-ss) with conductive metallic holes and fastened to the skull by small conductive screws (Pinnacle product #8209). An insulated tungsten wire (0.002”, California Fine Wire Company) was soldered to the EEG mount and trimmed to 2 mm to target the hippocampus (Klorig, Alberto et al. 2019), using epoxy to insulate the soldered portion of the electrode. The mount, with hippocampus electrode attached, was slowly lowered onto the skull with a micromanipulator such that the electrode was inserted directly down into the craniotomy over hippocampus. The headmount was then attached with a small amount of dental cement (C&B Metabond, Parkell) to hold the device steady as skull screws were then implanted into the remaining craniotomies. Skull screws were then reinforced to the headmount by conductive silver paint (SPI supplies). Dental cement (Metabond) was then used to cover all parts of the device and attach it firmly to the skull.

Recording and analysis

After recovery from surgery the headmount was attached to a preamplifier and animals placed in a bedded recording chamber with ad libitum food and water. Pinnacle EEG software recorded electrographic data at 400 Hz from the tethered preamplifier. Spontaneous activity was recorded for up to 5 hours, while heat-lamp experiments were recorded as described above. After recording, data were transferred to a PC and analyzed in MATLAB (Mathworks). Raw data were bandpass filtered (1-60 Hz, infinite impulse response filter with bandpass.m) and events of interest were automatically flagged by using line length of the signal (difference of successive voltage values with a moving 5-sec window), which permitted detection of large deviations (MATLAB findpeaks.m). Interictal and seizure events were then visually examined. In heat-lamp experiments, the times of temperature steps were recorded for alignment with the simultaneous EEG recording.

Hippocampal Neuronal Cultures

Hippocampi were dissected from P0-1 newborn pups and dissociated through enzymatic treatment with 0.25% trypsin and subsequent trituration. The cells were plated on glass coverslips previously coated with poly-D-lysine and laminin in 24-well cell culture plates. The hippocampal cells were grown in neurobasal A medium (ThermoFisher Scientific) supplemented with 2% B-27, 2mM glutamine, 10% heat-inactivated fetal bovine serum, and 1% penicillin/streptomycin in a 5% CO₂ incubator at 37°C overnight. After 24 hours this medium was replaced by a culture medium containing 2% B-27, 0.5mM glutamine, 1% heat-inactivated fetal bovine serum, 70 µm uridine and 25 µm 5-fluorodeoxyuridine. Cultured neurons were used for electrophysiology and immunocytochemistry.

Immunocytochemistry

Cells were fixed in 4% PFA 20 minutes, rinsed three times with phosphate buffered saline (PBS), and blocked in 2.5% bovine serum albumin with 0.2% Triton-X in PBS for 30 minutes. Primary anti-FGF13 antibody (Wang, Hennessey et al. 2011) was diluted in 2.5% bovine serum albumin and incubated in 4°C overnight. Coverslips were rinsed three times in PBS, then incubated in Alexa-568 secondary antibody (1:500 in 2.5% bovine serum albumin) for 1 hour at room temperature followed by DAPI for 5 minutes. Coverslips were mounted onto glass slides with mounting media (Vector Laboratories).

Acute Slice Preparation

Acute hippocampal slices were prepared from P12 to P14 mice. Briefly, after the mouse was anesthetized with isoflurane and then decapitated, the brain was quickly extracted and transferred into ice-cold cutting solution bubbled with 95% O₂ and 5% CO₂. The cutting solution contained (in mM): NaCl 77, sucrose 75, KCl 2.5, NaH₂PO₄ 1.4, NaHCO₃ 25, MgSO₄ 7, CaCl₂ 0.5, glucose 25, and sodium pyruvate 3, pH 7.4. Coronal brain slices (300 μm) including hippocampus were prepared using a Leica VT 1200S vibratome (Leica, Inc), and were incubated in a BSK-2 brain slice keeper (Automate Scientific, CA) containing oxygenated artificial cerebrospinal fluid (aCSF) at 35 °C for 30 min to recover. Afterwards, the slices were maintained at room temperature at least 30 min before use.

Electrophysiology

For spontaneous excitatory and inhibitory synaptic currents (sEPSCs and sIPSCs) in brain slices, the slice was placed in a recording chamber on the stage of an upright, infrared-differential interference contrast microscope (BX51WI, Olympus Optical) equipped with an ORCA-Flash2.8 C11440 Digital CMOS Camera (Hamamatsu Photonics), and was continuously perfused at a rate of 2 ml/min with aCSF bubbled with 95% O2 and 5% CO2 at 35°C. Pyramidal neurons in hippocampal CA1 stratum pyramidale were visualized with a 40X water-immersion objective. Spontaneous EPSCs and IPSCs were recorded in the whole-cell voltage clamp configuration at a holding potential of -70 mV and sampled at 10 kHz and filtered at 2 kHz using an Axopatch 200B amplifier and Digidata 1322A digitizer (Molecular Devices). The pipette internal solution for sEPSC contained (in mM): potassium gluconate (KGlu) 125, KCl 10, MgCl₂ 5, EGTA 0.6, HEPES 5, CaCl₂ 0.06, phosphocreatine disodium 10, Mg-ATP 2, Na₂-GTP 0.2, creatine phosphokinase 50 U/ml, and N-Ethyl lidocaine bromide 5, osmolarity 289 mOsm/L, pH 7.2 adjusted with KOH. The pipette internal solution for sIPSC contained (in mM): KCl 125, MgCl₂ 5, EGTA 0.6, HEPES 5, CaCl₂ 0.06, phosphocreatine disodium 10, Mg-ATP 2, Na₂-GTP 0.2, creatine phosphokinase 50 U/ml and N-Ethyl lidocaine bromide 5, osmolarity 291 mOsm/L, pH 7.2 adjusted with KOH. The external solution aCSF contained (in mM): NaCl 126, KCl 2.5, NaH₂PO₄ 1.25, NaHCO₃ 26, CaCl₂ 2, MgSO₄ 2, glucose 10. Bicuculline methiodide 20 μM was added to aCSF for sEPSC, and 2-amino-5-phosphonovaleric acid (APV) 50 μM and 6,7-dinitroquinoxaline-2,3-dione (DNQX) 20 μM was added to aCSF for sIPSC.

Whole-cell sodium Na⁺ currents and whole-cell K⁺ currents, or action potentials (APs) from cultured neurons were recorded with a HEKA EPC10 amplifier in the voltage-clamp or current-clamp configuration, respectively.

For Na⁺ current recordings in cultured neurons, the internal pipette solution contained (in mM): CsF 125, NaCl 10, HEPES 10, TEA-Cl 15, EGTA 1.1, Na-GTP 0.5, pH 7.4 with NaOH; the external solution contained NaCl 125, KCl 5, CaCl₂ 2, MgCl₂ 1, TEA-Cl 20, HEPES 5, Glucose 10, pH 7.4 with NaOH. For K+ current recordings and AP initiation in cultured neurons, the internal pipette solution contained (in mM): potassium gluconate 130, KCl 10, MgCl₂ 5, ethylene glycol-bis(β-aminoethyl ether)-N,N,N′,N′-tetraacetic acid 0.6, HEPES 5, CaCl₂ 0.06, phosphocreatine disodium 10, Mg-ATP 2, Na₂-GTP 0.2, and creatine phosphokinase 50 U/ml, pH 7.2 adjusted with KOH; the external solution contained (in mM): NaCl 119, KCl 5, HEPES 20, CaCl₂ 2, MgCl₂ 2, glucose 30, APV 0.05, DNQX 0.02, bicuculline 0.02, pH 7.3 adjusted with NaOH. Additionally for K+ current recordings, the external solution contained 100 nM tetrodotoxin (TTX) and 5 µM nifedipine to block Na⁺ and Ca²⁺ channels.

Recording pipettes were pulled from borosilicate glass with Sutter P-97 Micropipette Puller (Sutter Instrument Co.). For Na⁺ and K⁺ current recordings, pipette resistance ranged from 1.5 to 2.5 MΩ and the series resistance was compensated by at least 70%. For AP initiation recordings, pipette resistance ranged from 2.0 to 3.0 MΩ. For recordings of sEPSCs and sIPSCs in brain slices, pipette resistance ranged from 2.6 to 6.1 MΩ and series resistance was 10.5 ± 0.5 MΩ for WT and 10.8 ± 0.4 MΩ for Gad2^{Fgf13 KO} without compensation.

Analysis of Electrophysiological Data

Action potentials were elicited by holding the cell at 0 pA in current clamp mode and then stimulating with current increments for 1 s. The numbers of action potentials elicited for each current injection were quantified using Fitmaster software. Action potential parameters were analyzed using Clampfit 10.4 software. Specifically, action potential amplitude and action potential duration measured at 50% of the amplitude (APD50) values for the first three action potentials were determined using the statistics function. Additionally, dV/dt values were computed using the differential function. The threshold potential was determined by analyzing the phase plot of the initial action potential at rheobase by identifying the voltage value on the x-axis where the y-axis reached a rate of 1 mV/ms.

Na⁺ and K⁺ channel currents were activated by holding the neuron at -90mV and applying incremental voltages for a duration of 150 ms. Fitmaster software was used for the quantification of various channel parameters. The non-inactivating portion of the K⁺ channel current was assessed by analyzing the peak current at the conclusion of 150 ms depolarizing pulses. To generate steady-state inactivation curves, currents were elicited at a holding potential of -120 mV followed by a 500-ms prepulse to voltages ranging from -120 to +20 mV. Subsequently, currents were measured at -20 mV for 20 ms. Normalized current values obtained at -20 mV were utilized to construct the steady-state inactivation curves. A Boltzmann equation, [I/Imax = (1 + exp ((V − V1/2) / k))−1], was employed to fit the data, where Imax denotes the maximum current, V1/2 represents the half-inactivation voltage, and k signifies the slope. This equation facilitated the calculation of V1/2 of inactivation.

Data for Na⁺ and K⁺ current or APs were analyzed with Axon Clampfit (Molecular Devices), and data for sEPSC and sIPSC were analyzed with Mini Analysis (Synaptosoft).

Immunohistochemistry

Mice were sacrificed at postnatal day 13-16 (P13-16). Brains were extracted after transcardial perfusion of PBS followed by 4% paraformaldehyde (PFA). They were incubated overnight rocking at 4 °C in 4% paraformaldehyde, then equilibrated in 15% sucrose followed by 30% sucrose. Brains were embedded in Optimal Cutting Temperature (OCT) compound in cryomolds and cryosectioned at 50 µm into 0.1 M PBS. Floating sections were washed 3 times with PBS, then blocked for 1 hour in 2.5% bovine serum albumin and 0.2% Triton-X in PBS. Tissue was incubated with the anti-FGF13 antibody overnight at 4°C. After sections were washed three times with PBS, they were incubated with Alexa-568 secondary antibody for 2 hours at room temperature. Sections mounted onto glass slides with mounting media (Vector laboratories) and sealed with glass cover slips. Slides were stored at 4 °C. Hippocampal tissue was imaged using a confocal microscope (Zeiss LSM 880) and analyzed using Image-J software.

Western Blot

Tissue was immersed in ice cold RIPA buffer supplemented with Halt protease and phosphatase inhibitor cocktails (Thermo Fisher Scientific) and placed in a manual Dounce tissue homogenizer, in which they were homogenized for 1 minute on ice. The homogenate was then centrifuged at 21,000 x g at 4 °C. Supernatant was collected and protein concentration was determined by bicinchoninic acid assay. Protein was separated on an 8-16% gradient Tris-glycine gels and transferred to PVDF blotting membrane (GE Healthcare Life Sciences). The membrane was immunoblotted with 1:200 anti-FGF13 antibody or 1:200 anti-pan FHF-A (Neuromab clone N235/22) for two hours at RT to immunoblot for FGF13-S. Vinculin (Sigma V9131) was used as a loading control. The blots were visualized by chemiluminescence and images were captured using ChemiDoc^TM Tough Imaging System (BioRad).

BaseScope in situ hybridization

Mice were sacrificed at P13-15. Brains were extracted after transcardial perfusion of PBS followed by 4% paraformaldehyde. The tissue was incubated for 24 hours rocking at 4°C in 4% paraformaldehyde, then equilibrated in 15% sucrose followed by 30% sucrose. Brains were embedded in OCT compound in cryomolds and sectioned coronally in 14 µm sections onto SuperFrost (ThermoFisher) slides, then stored at -80°C up to three months. Custom Fgf13 isoform probes were generated as previously described (Joglekar, Prjibelski et al. 2021) and used according to the manufacturer’s protocol for fixed frozen tissues. Hematoxylin followed by 0.02% ammonia water was used for nuclear counterstain.

Targeted metabolomics

Mice were sacrificed at P13 and brains were immediately extracted, homogenized, and placed into pre-chilled 80% methanol (-80L°C). The extract was dried with a Speedvac, and redissolved in HPLC grade water before it was applied to the hydrophilic interaction chromatography LC-MS. Metabolites were measured on a Q Exactive Orbitrap mass spectrometer (Thermo Scientific), which was coupled to a Vanquish UPLC system (Thermo Scientific) via an Ion Max ion source with a HESI II probe (Thermo Scientific). A Sequant ZIC-pHILIC column (2.1 mm i.d. × 150 mm, particle size of 5Lµm, Millipore Sigma) was used for separation of metabolites. A 2.1L×L20Lmm guard column with the same packing material was used for protection of the analytical column. Flow rate was set at 150 μL/min. Buffers consisted of 100% acetonitrile for mobile phase A, and 0.1% NH₄OH/20 mM CH₃COONH₄ in water for mobile phase B. The chromatographic gradient ran from 85% to 30% A in 20 min followed by a wash with 30% A and re-equilibration at 85% A. The Q Exactive was operated in full scan, polarity-switching mode with the following parameters: the spray voltage 3.0LkV, the heated capillary temperature 300L°C, the HESI probe temperature 350L°C, the sheath gas flow 40 units, the auxiliary gas flow 15 units. MS data acquisition was performed in the m/z range of 70–1,000, with 70,000 resolution (at 200 m/z). The AGC target was 1e6 and the maximum injection time was 250 ms. The MS data was processed using Xcalibur 4.1 (Thermo Scientific) to obtain the metabolite signal intensities. Identification required exact mass (within 5 ppm) and standard retention times. Statistical analysis was performed as follows: The intensity values were subjected to a Log2 transformation to normalize the data distribution. Student’s t-test was conducted to calculate the significance of observed differences between groups. Enrichment analyses were performed using Metabolanalyst online tools (https://www.metaboanalyst.ca/).

Reverse transcriptase quantitative polymerase chain reaction

From hippocampal neuron cutlures prepared for electrophysiology, RNA was isolated using RNeasy Mini Kit (QIAGEN) according to the manufacture’s instructions. Reverse transcription to generate cDNA was performed using SuperScript^TM IV VILO^TM Master Mix with ezDNase (Invitrogen). qPCR was performed in duplicate for each sample with QantStudio 3 (Applied Biosystems) using SYBR green-based detection chemistries (Bio-Rad). For primer sequences used for qPCR target genes, see Supplemental Table 1.

Statistics

Statistical analyses were performed in GraphPad Prism v10 and specific analyses are described in the accompanying figure legends.

Results

Whole brain knockout of Fgf13 results in spontaneous seizures and premature death

To determine how FGF13 affects neuronal excitability and provide insight into how FGF13 variants contributes to seizure disorders, we developed genetic mouse models that eliminate Fgf13 in specific neuronal cell types. We started by eliminating the X-linked Fgf13 in all neurons, crossing a male Nestin-Cre driver with a Fgf13^fl/fl female mouse from a previously validated line (Wang, Tang et al. 2017) (Figure 1A) to generate hemizygous male Fgf13 knockouts (Nes-cre;Fgf13^fl/Yor “Nestin^{Fgf13 KO}”) and heterozygous females (Fgf13^fl/+ or “Nestin^{Fgf13 HET}”) alongside wild type (WT) littermates. We validated our mouse lines by examining the hippocampus, where Fgf13 is highly expressed (Pablo, Wang et al. 2016) and which has previously been implicated in FGF13-related seizure pathology (Puranam, He et al. 2015, Shen, Yue et al. 2022) and cognition (Wu, Yang et al. 2012). In hippocampus from WT mice, western blotting with a pan-FGF13 antibody that recognizes all FGF13 isoforms detected four distinct bands that we were able to assign to specific FGF13 isoforms by running standards (isoform specific cDNAs expressed in HEK293 cells) (Figure 1B and Supplemental Figure 1A-B). In hippocampi from Nestin^{Fgf13 KO}brains we observed near complete absence of FGF13 (Figure 1B) by western blot and by immunohistochemistry (Figure 1C). In WT mice, FGF13 signal is prominent in the hippocampal pyramidal cell layer as well as in sparse presumed interneuron somata (see below) throughout all layers. Offspring were born at expected Mendelian ratios (Table 1), but all Nestin^{Fgf13 KO} male mice died before weaning with a median survival age of 17 days postnatal (P17; Figure 1D). Nestin^{Fgf13 HET}females also exhibited postnatal death, with only 60% surviving past one month (Figure 1D), implying a gene dosage effect of Fgf13 loss. Nestin^{Fgf13 KO} male mice suffered spontaneous seizures in their home cage (Supplemental video 1) as early as P12, followed by premature death (Figure 1D), consistent with mouse models of DEE that exhibit SUDEP (Bunton-Stasyshyn, Wagnon et al. 2019, Han, Chen et al. 2020). Nestin^{Fgf13 KO} males were smaller than their wild type littermates by P14 (Figure 1E), suggesting developmental delay, likely a consequence of recurrent seizures and consistent with DEE mouse models (Yu, Mantegazza et al. 2006, Kalume, Westenbroek et al. 2013, Teran, Sainju et al. 2023).

Figure 1.

Table 1:

As febrile seizures are a hallmark of early developmental onset epilepsy and were observed in subjects with a gene translocation that disrupted the FGF13 locus (Puranam, He et al. 2015), we tested hyperthermia-induced seizure susceptibility in the Nestin^{Fgf13 KO} male mice, following a modified protocol (Cheah, Yu et al. 2012, Puranam, He et al. 2015). Mice were tested at P12, the age at which we first observed spontaneous home cage seizures. Briefly, mice were acclimated to the testing chamber and a heat lamp was used to increase core body temperature at a steady rate of 0.5 °C every 2 minutes until 42.0 °C to simulate fever onset. All Nestin^{Fgf13 KO}males exhibited tonic-clonic seizures during the hyperthermic seizure protocol while wild type mice remained seizure free (Figure 1F).

Excitatory neuronal knockout of Fgf13 does not result in spontaneous seizures

Excitatory neurons have been the focus of most studies investigating Fgf13 dysfunction. Fgf13 deficiency in excitatory forebrain neurons is linked to neurodevelopmental delay and cognitive impairment (Wu, Yang et al. 2012), and excitatory neurons are hypothesized to be the relevant cell type for seizures in a DEE associated with FGF13 variants (Fry, Marra et al. 2021). To test the contribution of excitatory neurons to the seizure and SUDEP phenotype identified in Nestin^{Fgf13 KO} mice, we generated an excitatory neuron-targeted knockout mouse using an Emx1-Cre driver (Gorski, Talley et al. 2002). We assessed efficacy of knockout by western blot using the pan-FGF13 antibody. In Emx1^{Fgf13 KO} mice, western blots showed the loss of two FGF13 isoforms (Figure 2A), FGF13-S and FGF13-U, consistent with single-cell long-read RNA sequencing that showed that excitatory neurons predominantly express FGF13-S (Joglekar, Prjibelski et al. 2021), which we confirmed with a FGF13-S specific antibody (Supplemental Figure 1C). FGF13-VY and FGF13-V, the major isoforms expressed in inhibitory interneurons (Joglekar, Prjibelski et al. 2021), were preserved. Thus, these data confirm at the protein level the differential expression of specific Fgf13 transcripts in excitatory vs. inhibitory neurons observed by single cell RNA sequencing. Fluorescent immunohistochemistry of hippocampi from Emx1^{Fgf13 KO} showed loss of FGF13 from the CA1 pyramidal cell layer but maintenance of FGF13 signal from sparse putative interneuron somata (Figure 2B). Emx1^{Fgf13 KO} mice were born at expected Mendelian ratios (Table 1) and all survived to adulthood (Figure 2C), similar to a previous report (Wu, Yang et al. 2012). Average body size and mass at P14 revealed no differences between wild type and Emx1^{Fgf13 KO}genotypes (Figure 2D). None of the Emx1^{Fgf13 KO} succumbed to seizures during the hyperthermia protocol (Figure 2E), and EEG recordings during the hyperthermia protocol confirmed no seizure activity in Emx1^{Fgf13 KO} or wild type mice (Figure 2F). These data show that loss of Fgf13 from excitatory forebrain neurons is not sufficient to induce seizure susceptibility.

Figure 2.

The mechanism by which DEE-associated variants in FGF13-S contribute to a pro-excitatory state and seizures was hypothesized to be loss of a FGF13-S dependent long-term inactivation, a process that describes a successive reduction in peak Na_V current following repetitive depolarizations and is thought to derive from accreting channel pore blockade by the alternatively spliced N-terminus of FGF13-S (Fry, Marra et al. 2021). Whether FGF13-S confers long-term inactivation in neurons has not been demonstrated. We employed the knockout model to assess the effects of FGF13-S on Na_V currents in Emx1⁺excitatory neurons and determine if FGF13-S bestows long-term inactivation. We cultured hippocampal neurons from Emx1^{Fgf13 KO} or wild type littermates (Emx-Cre) and infected them with a Cre-dependent AAV8-DIO-GFP virus to allow identification of the Emx1⁺ neurons by GFP (Supplemental Figure 2A). The major neuronal voltage gated sodium channels (Na_V1.1, Na_V1.2, Na_V1.3, and Na_V1.6) are expressed in these neuron cultures consistent with levels previously reported (Heighway, Sedo et al. 2022), as assessed by reverse transcriptase quantitative polymerase chain reaction (Supplemental Figure 2B). Current density and the I-V relationship were not different between WT and Emx1^{Fgf13 KO}neurons (Supplemental Figure 2C), and the V_1/2 of steady-state inactivation was not significantly different in Emx1^{Fgf13 KO} neurons compared to WT controls (Supplemental Figure 2D). To assess for long-term inactivation, we applied successive depolarizations (Figure 2G) and observed successive reductions in peak current in WT neurons, a process blunted in Emx1^{Fgf13 KO}neurons. Thus, although Fgf13 ablation in Emx1⁺ neurons diminished long-term inactivation—similar to that observed for DEE associated variants in FGF13-S expressed in Neuro2A cells (Fry, Marra et al. 2021)—these data suggest that FGF13-S dysfunction in excitatory neurons is an unlikely contributor to a pro-excitatory state and seizures.

Inhibitory neuron knockout of Fgf13 recapitulates spontaneous seizures and premature death in complete neuronal knockout

Since Fgf13 knockout in excitatory neurons did not recapitulate the seizure phenotype seen in the Nestin^{Fgf13 KO} animals, we suspected that absence of Fgf13 specifically in inhibitory interneurons may be playing the critical role. With immunohistochemistry on brains from mice in which a Gad2-Cre driver (Taniguchi, He et al. 2011) expressed a Cre-dependent GFP (Ai6) reporter (Madisen, Zwingman et al. 2010) in inhibitory interneurons (Supplemental Figure 3A-B), one-third of the GFP⁺ interneurons expressed FGF13 at P13 (Figure 3A). We eliminated Fgf13 specifically in inhibitory neurons by crossing the Gad2-Cre driver and Fgf13^fl/fl mice. The FGF13 signal by immunohistochemistry was completely eliminated from the GFP⁺ cells in mouse brains also expressing GFP from the Gad2-Cre driver while the diffuse staining pattern in the excitatory pyramidal cell layer and overall hippocampal morphology were unaffected (Supplemental Figure 3A-B). Further, higher magnification images showed that in Gad2^{Fgf13 KO} mice the FGF13⁺ staining in sparse somata (presumed interneurons above) was completely eliminated (Figure 3B). Western blots with the pan-FGF13 antibody showed partial depletion of FGF13 in Gad2^{Fgf13 KO} (Figure 3C), with the most significant reduction in FGF13-VY and FGF13-Y while FGF13-S was partially spared, consistent with our analysis of splice-variant specific transcript data (Joglekar, Prjibelski et al. 2021).

Figure 3.

In conjunction with the generation of the Nestin^{Fgf13 KO} and Emx1^{Fgf13 KO} mice, the Gad2^{Fgf13 KO} mice provided the opportunity to validate and extend the previously published transcript data (Joglekar, Prjibelski et al. 2021) and the protein (western blots in this study) data in cell type-specific knockout models. Using BaseScope in situ hybridization we characterized Fgf13-S and Fgf13-VY expression in intact hippocampi on fixed frozen tissue. We detected diffuse Fgf13-S expression in excitatory cell layers while Fgf13-VY expression was concentrated in interneuron somata in wild type hippocampi (Supplemental Figure 4A-B). Quantification of the mRNA signal intensity revealed a decrease in Fgf13-S for genotypes in which we deleted Fgf13 in excitatory cells (Nestin^{Fgf13 KO} and Emx1^{Fgf13 KO}); meanwhile quantification of the cell somata expressing Fgf13-VY revealed a decrease in the Fgf13-VY⁺ cell count for genotypes in which we deleted Fgf13 in interneurons (Nestin^{Fgf13 KO} and Gad2^{Fgf13 KO}), as shown in Supplemental Figure 4C. In situ hybridization in these knockout models confirms the splice variant-specific transcript data previously obtained (Joglekar, Prjibelski et al. 2021), although we did not detect the expected decrease in the Fgf13-S signal in Gad2^{Fgf13 KO} mice, likely because we lacked the resolution due to the overwhelming Fgf13-S signal from excitatory neurons.

With this confirmation, we investigated the consequences of Fgf13 loss from interneurons. None of the male Gad2^{Fgf13 KO} hemizygous knockout mice survived to adulthood (Figure 3D), similar to the Nestin^{Fgf13 KO} male mice. The median survival in male Gad2^{Fgf13 KO} mice was 14.5 days, and survivors at P14 were smaller than their wild type littermates (Figure 3E). Female Gad2^{Fgf13 KO}mice also had a survival deficit (Figure 3D), though less severe than their male knockout littermates, suggesting a gene dosage effect. Brains of male Gad2^{Fgf13 KO}mice were smaller compared to wild type littermates, as was body size (Figure 3E).

Interneuron-specific knockout of Fgf13 increased susceptibility to seizures in the hyperthermia-induced seizure protocol. All Gad2^{Fgf13 KO} males suffered tonic-clonic seizures while wild type littermates did not (Figure 3F-G). Furthermore, we observed some Gad2^{Fgf13 KO} males were susceptible to seizures during acclimation to the testing chamber, prior to the initiation of the hyperthermia protocol. With witnessed seizures immediately preceding death in some mice, we interpret that the previously noted unwitnessed premature deaths in the home cage were likely related to recurrent seizures. Together, these data suggest that FGF13 deficiency in inhibitory cells, rather than excitatory cells, is the major contributor to the seizures and premature mortality seen in the Nestin^{Fgf13 KO} mice.

Given the seizures and mortality in the Gad2^{Fgf13 KO} mice and because seizures can be associated with neuronal death (Henshall and Simon 2005), we considered if Fgf13 ablation led to loss of hippocampal interneurons. We quantified Gad2-GFP⁺ interneurons in Gad2^GFP(Gad2^GFP vs. Gad2^{GFP-Fgf13 KO}) mice, in which Gad2 drove both Fgf13 ablation and expression of a GFP reporter. We found no difference in the number of Gad2-GFP⁺ hippocampal neurons between genotypes (Supplemental Figure 3C), indicating that Gad2^{Fgf13 KO} mice did not have a deficit of interneurons underlying their seizure phenotype. Further, an unbiased metabolomic analysis on brains from Gad2^{Fgf13 KO} and WT control mice revealed marked differences between genotypes (Supplemental Figure 5A and Supplemental Table 2) and several features consistent with severe seizures. For example, the metabolite most enriched in Gad2^{Fgf13 KO} brains was L-kynurenine (Log₂fold change = 2.58, P= 0.0009), a metabolite most enriched in patients with status epilepticus (Hanin, Chollet et al. 2024). Metabolite set enrichment analysis in Gad2^{Fgf13 KO} vs. WT (Supplemental Table 2) revealed that the most enriched Kyoto Encyclopedia of Genes and Genomes (KEGG) pathway among upregulated metabolites was glycolysis (P=4.29E-6), also consistent with data obtained in patients in status epilepticus (Hanin, Chollet et al. 2024). The most downregulated pathway was methionine metabolism (P=9.88E-4), consistent with methionine synthase deficiency—an inborn error of metabolism—that present with seizures (Kripps, Sremba et al. 2022). Thus, this metabolomic analysis supported the severity of the seizure phenotype observed in Gad2^{Fgf13 KO}mice.

MGE-derived interneuron knockout of Fgf13 partially recapitulates spontaneous seizures and premature death

As not all Gad2⁺ interneurons express Fgf13 (Supplemental Figure 3A), we analyzed a single cell RNA-seq dataset from mouse CA1 interneurons (Harris, Hochgerner et al. 2018) to search for a subpopulation functionally relevant to the seizure pathology. We found the highest enrichment of Fgf13 in subsets assigned as axo-axonic and medial ganglionic eminence (MGE) neurogliaform/Ivy cells (Supplemental Figure 6A-B) expressing the homeodomain transcription factor Nkx2.1. Further, Fgf13 expression has previously been identified in Nkx2.1⁺ MGE-derived interneurons, including axo-axonic chandelier cells (Paul, Crow et al. 2017, Mahadevan, Mitra et al. 2021), which depend upon Fgf13 expression for proper development (Favuzzi, Deogracias et al. 2019). Single-cell profiling of human postmortem cortical tissue has identified high FGF13 expression in neurogliaform and parvalbumin interneurons throughout early development (Herring, Simmons et al. 2022). While Fgf13 expression was not completely restricted to Nkx2.1⁺MGE-derived interneurons, we thus chose an Nkx2.1-Cre driver (Xu, Tam et al. 2008) to target Fgf13 deletion from interneurons generated in the MGE.

Fluorescent immunohistochemistry in brain slices from Nkx2.1^{Fgf13 KO} mice showed partial depletion of the sparse somatic distribution of FGF13⁺ somata observed in the Gad2^{Fgf13 KO}mice (Supplemental Figure 6C). Consistent with that result, BaseScope in situ hybridization in Nkx2.1^{Fgf13 KO} mice showed a pattern similar to Gad2^{Fgf13 KO}mice but with less complete loss of the interneuron somata (Supplemental Figure S4B). Nkx2.1^{Fgf13 KO}mice were born at expected Mendelian ratios (Table 1) but only ∼ 40% of male Nkx2.1^{Fgf13 KO} mice survived past one month of age (Supplemental Figure 6D), consistent with a partial loss of FGF13 expression in hippocampal interneurons (Supplemental Figure 6C). The median survival age for male Nkx2.1^{Fgf13 KO} mice was 22 days (P22), and surviving mutants were smaller than their wild type littermates at P14 (Supplemental Figure 6E). Female Nkx2.1^{Fgf13 HET} survived to adulthood. We found that almost all male Nkx2.1^{Fgf13 KO}suffered tonic-clonic seizures during the hyperthermia induction protocol, while wild type littermates did not (Supplemental Figure 6F). Because the lethality and seizure susceptibility in the Nkx2.1^{Fgf13 KO} mice were reduced compared to the Gad2^{Fgf13 KO}mice, we hypothesize that MGE-derived neurons are partially responsible for the phenotype observed in Gad2^{Fgf13 KO} mice. The loss of FGF13 from other interneuron classes in which FGF13 is expressed—as evident from single cell RNA sequencing (Supplemental Figure 6A-B)—likely contributes to the more severe phenotype after broader inhibitory interneuron knockout by the Gad2-Cre driver.

Inhibitory neuronal knockout of Fgf13 results in deficits of synaptic transmission

To identify if the seizure susceptibility of the Gad2^{Fgf13 KO} mice is caused by loss of excitatory/inhibitory balance in the hippocampus, we recorded spontaneous excitatory and inhibitory inputs to the CA1 pyramidal cells of the dorsal hippocampus in slice recordings. Pyramidal cells in Gad2^{Fgf13 KO} hippocampi, compared to wild type littermates, showed an increased frequency of sEPSCs (Figure 4A-B) and a decreased frequency of sIPSCs mice relative to wild type littermates (Figure 4C-D). Because there was no significant change in sEPSC or sIPSC amplitude (Figure 4B, D), the increased sEPSC and decreased sIPSC frequencies indicate a presynaptic and not postsynaptic mechanism. Together, these data suggest that ablation of Fgf13 specifically in inhibitory neurons (in Gad2^{Fgf13 KO} mice) decreased direct and downstream inhibitory drive onto pyramidal cells, thereby increasing pyramidal cell excitability.

Figure 4.

Inhibitory neuronal knockout of Fgf13 results in deficits of interneuron excitability

To assess the cellular mechanisms underlying decreased inhibitory drive from the inhibitory neurons in Gad2^{Fgf13 KO} mice, we cultured hippocampal neurons from Gad2^{Fgf13 KO} or wild type littermates (Gad2-Cre) and infected them with a Cre-dependent AAV8-DIO-GFP virus, thus allowing identification of the Gad2⁺ interneurons by GFP (Figure 5A). We quantified trains of action potentials in response to current injection in the GFP⁺ neurons to assess intrinsic excitability. Increasing current injection augmented the number of spikes in WT (Gad2-Cre) neurons until a plateau at ∼260 pA (Figure 5B). At low levels (<100 pA) current injection elicited a similar number of spikes in neurons from Gad2^{Fgf13 KO}mice (albeit spike morphology and frequency were different, see below) but the number of spikes then plateaued and was less than the number elicited in neurons from WT mice at higher amounts of current injection (Figure 5B), suggesting a decrease in intrinsic excitability in neurons from Gad2^{Fgf13 KO} mice. Examination of individual traces revealed that more Gad2^{Fgf13 KO} cells entered depolarization block, and at lower levels of current injection than wildtype interneurons (Figure 5C). The detected difference between genotypes is striking considering that only a third of the Gad2⁺ neurons from Gad2^{Fgf13 KO} infected with the Cre virus would be expected to express FGF13 before viral Cre expression (Figure 3A).

Figure 5.

To further investigate the mechanisms contributing to decreased excitability and depolarization block, we examined the first elicited action potential properties for each spike train at rheobase. Resting membrane potential, rheobase, and threshold potential were not different between genotypes, Figure 5D. The single action potential wave forms and phase plots show little difference between Gad2^{Fgf13 KO} neurons infected with the Cre virus and wild type controls (Figure 5E), although action potential duration measured at 50% of the amplitude (APD50) trended longer in the Gad2^{Fgf13 KO}interneurons infected with the Cre virus (Supplemental Figure 7A). However, we observed marked genotype differences in the second and third elicited action potentials. Most notably, in Gad2^{Fgf13 KO} interneurons we observed a progressive reduction in the action potential peak amplitude and dV/dt max, an increase in APD50, and a greater increase in the interspike membrane voltage (Figure 5F-G), suggesting a growing repolarization deficit in the Gad2^{Fgf13 KO} neurons each subsequent spike, thus increasing the likelihood to undergo depolarization block.

Since the first spike action potential parameters were not significantly different between Gad2^{Fgf13 KO} neurons and wild type controls, we hypothesized that loss of FGF13 had minimal effects upon Na_V channel currents in these neurons. Indeed, we observed no differences in current amplitude nor steady-state inactivation between Gad2^{Fgf13 KO} neurons and wild type controls (Supplemental Figure 7B, C). Because we did not detect significant differences in Na_V current properties typically associated with FGF13 in Fgf13 knockout in Gad2^{Fgf13 KO}neurons, we hypothesized that FGF13 regulated other currents that led to the observed changes in action potentials and decrease in repolarization. Since in cardiomyocytes we showed that FGF13 can also affect various K_V channels that contribute to the repolarizing phase of the cardiac action potential (Wang, Tang et al. 2017), here we recorded macroscopic potassium currents and observed a reduced Kv current density in Gad2^{Fgf13 KO} interneurons compared to WT neurons (Figure 5I).

Virally mediated re-expression of Fgf13-S and Fgf13-VY restores output to Gad2^{Fgf13 KO} neurons

Since inhibitory neurons express both Fgf13-S and Fgf13-VY, we tested if re-expression of either of these isoforms in Gad2^{Fgf13 KO} neurons could rescue the observed deficit in the input/output relationship. We isolated primary hippocampal neurons from Gad2^{Fgf13 KO} or controls (Gad2-Cre) and infected them with the Cre-dependent AAV8-DIO-GFP virus along with either an AAV8-DIO-Fgf13-S or AAV8-DIO-Fgf13-VY. Immunocytochemistry of GFP⁺ neurons showed expression of endogenous FGF13 in Gad2-Cre cultures and the absence of FGF13 in Gad2^{Fgf13 KO}cultures (Figure 6A). Infection with Fgf13-S in a Gad2^{Fgf13 KO} neuron showed concentrated expression in the axon initial segment and membrane-enriched signal in the soma and the dendritic branches (Figure 6A) while infection with Fgf13-VY produced prominent signal throughout the soma and branches, demonstrating successful re-expression of these splice variants in the knockout background. After viral re-expression of Fgf13-VY or Fgf13-S, neither threshold potential nor rheobase were affected and were not different compared to values from either WT or Gad2^{Fgf13 KO} neurons (Figure 6B). After rescue with either Fgf13-VY or Fgf13-S, current injection >100 pA elicited more action potentials than in Gad2^{Fgf13 KO} neurons, suggesting that excitability was at least partially restored (Figure 6C). Indeed, compared to Gad2^{Fgf13 KO} neurons a smaller fraction of Gad2⁺ cells re-expressing Fgf13-VY or Fgf13-S reached depolarization block when injected with >100 pA (Figure 6D), although neither Fgf13-VY nor Fgf13-S alone reduced the probability of conduction block to what was observed in WT neurons. Further analysis showed that, even though Fgf13-S or Fgf13-VY partially restored spiking, the action potential wave forms and the phase plots were not restored by either Fgf13-S or Fgf13-VY alone (Figure 6E). Examination of specific parameters revealed that neither Fgf13-S nor Fgf13-VY rescue was able to prevent the prolongation of APD50 nor reduction in the action potential amplitude, dV/dt max or action potential peak amplitude observed in Gad2^{Fgf13 KO} neurons (Figure 6F), again suggesting that neither FGF13-S nor FGF13-VY is sufficient for maintaining excitability in Gad2 neurons. On the other hand, infection with Fgf13-S partially hyperpolarized the interspike membrane potential (compared to Gad2^{Fgf13 KO}, Figure 6G), suggesting that FGF13-S increased the repolarizing K⁺ currents. Indeed, infection with Fgf13-S but not Fgf13-VY increased K⁺ current density to WT levels (Figure 6H). These data suggest that FGF13-S and FGF13-VY, both expressed in inhibitory interneurons (Joglekar, Prjibelski et al. 2021) contribute to inhibitory interneuron function and modulation of pyramidal neuron excitability.

Figure 6.

Discussion

While variants in or disruption of FGF13 have been associated with DEEs (Puranam, He et al. 2015, Fry, Marra et al. 2021, Velíšková, Marra et al. 2021, Narayanan, Majethia et al. 2022), the pathogenesis was unknown. Employing multiple cell type specific mouse knockout models complemented by isoform specific rescue strategies, our data reveal how FGF13 ablation contribute to seizure susceptibility and provide new insights into FGF13 functions in neurons. We found that Fgf13 ablation and consequent loss of FGF13-S and FGF13-VY in a subset of interneurons reduced overall inhibitory drive from Fgf13-expressing interneurons onto hippocampal pyramidal neurons. Rescue experiments suggest that both FGF13-S and FGF13-VY isoforms are required for proper interneuron function as re-expression of FGF13-S or FGF13-VY only partially restored excitability (our experimental setup did not allow rescue with both isoforms simultaneously). Building upon our recent analysis of Fgf13 splice variant expression (Joglekar, Prjibelski et al. 2021), our data resolve apparently conflicting reports in which reduced inhibitory interneuron function, suggested as the main contributor in a global Fgf13 female heterozygous knockout model, (Puranam, He et al. 2015) contrasts with a model that proposes that FGF13 variants within excitatory neurons drive increased excitability because of diminished long-term inactivation (Fry, Marra et al. 2021).

The apparent requirement of both FGF13-S and FGF13-VY extends previous studies showing their distinct roles in neurons (Pablo, Wang et al. 2016) and emphasizes that alternative splicing is an important source of protein diversity in the mammalian brain, an evolutionarily conserved feature thought to contribute to the nervous system’s complexity (Raj and Blencowe 2015, Zhang, Chen et al. 2016, Karlsson and Linnarsson 2017, Porter, Jaamour et al. 2018, Furlanis, Traunmuller et al. 2019, Joglekar, Foord et al. 2023). Cell-specific alternative splicing in the brain has been posited as a mechanism to efficiently adapt to the external environment by quickly modifying protein activity (Lipscombe and Lopez Soto 2019). Not only does FGF13 have the most extensive set of alternatively spliced isoforms among FHFs (Smallwood, Munoz-Sanjuan et al. 1996, Munoz-Sanjuan, Smallwood et al. 2000, Pablo, Wang et al. 2016), but long-range single cell sequencing data show that Fgf13 has a uniquely (among FHFs) segregated alternative splice variant expression pattern among distinct neuron cell type. Further, among all genes, has one of the highest differential isoform expression (DIE) values across multiple neuronal cell-types (Joglekar, Prjibelski et al. 2021).

Our results are also consistent with the available patient data. The responsible splice variant(s) were proposed to be either FGF13-V, FGF13-VY, and FGF13-Y that were lost in two affected brothers who inherited a maternal balanced translocation that disrupts FGF13 on the X-chromosome and preserves the FGF13-S and the FGF13-U splice variants (Puranam, He et al. 2015) or, in contrast, FGF13-S in a series of unrelated individuals presenting with DEE symptoms (Fry, Marra et al. 2021). As our data suggest that both FGF13-S and FGF13-VY contribute within inhibitory interneurons, we provide a unifying explanation for those reports. Here, we were able to assess FGF13-S and FGF13-VY, chosen because they are most abundantly expressed isoforms in the adult mouse brain, but the inability to rescue electrophysiological consequences completely with either isoform alone leaves open the possibility that other isoforms (e.g., FGF13-U, FGF13-V) also make critical contributions.

These results also expand our understanding of how FGF13 contributes to neuronal functions, which have been challenging to define because of FGF13’s location on the X chromosome, the embryonic lethality of complete knockout models, absence of cell-type specific knockout models, FGF13’s complex alternative splicing, and an incomplete cataloging of specific functions for the various isoforms generated. Various roles for FGF13 in inhibitory interneurons have previously been suggested. Fgf13 silencing in Nkx2.1-CreER targeted neurons reduced the number of chandelier cell boutons (Favuzzi, Deogracias et al. 2019) and a more general role for FGF13 in interneuron development was suggested by a human scRNA-seq dataset (Herring, Simmons et al. 2022). Our data here, in which seizure susceptibility was attributable solely to Fgf13 knockout in inhibitory interneurons and our demonstration that Fgf13 knockout restricted to Nkx2.1-expressing neurons increased seizure susceptibility—albeit to a lesser extent than complete knockout in inhibitory interneurons—support not only a possible role for Fgf13 in chandelier cell development but also confirm more general inhibitory interneuron roles. Along with the reduced seizure susceptibility of female heterozygote knockout animals, these data also imply a gene dosage effect within interneurons. The differences in survival among Gad2^{Fgf13 KO}, Gad2^{Fgf13 HET}, Nkx2.1^{Fgf13 KO}, and Nkx2.1^{Fgf13 HET} also suggest a gene-dosage effect. Although we were unable to generate female homozygous Gad2^{Fgf13 KO} mice since the male hemizygous knockouts did not survive to adulthood, the reduced survival in male knockouts compared to female heterozygous knockouts further supports our hypothesis. The relative comprehensiveness of the specific Cre drivers also provides support for our hypothesis. In the hyperthermic seizure assay, mice from both the Nestin^{Fgf13 KO} and Gad2^{Fgf13 KO} lines, in which Fgf13 was ablated in the entire interneuron population, suffered seizures at baseline (near 36 °C) as well as at elevated core body temperatures. In contrast, the majority of the Nkx2.1^{Fgf13 KO} mice, generated with a more restrictive Cre driver, mostly suffered seizures only at elevated core body temperatures. We also observed occasional seizures in the home cage for all genotypes in which Fgf13 was ablated in interneurons (Nestin^{Fgf13 KO}, Nkx2.1^{Fgf13 KO}, and Gad2^{Fgf13 KO}) and often discovered dead mice, which we suspect was a SUDEP phenotype due to recurrent seizures, given that recurrent uncontrolled seizures are a major risk factor for sudden death (Devinsky, Hesdorffer et al. 2016, Richerson 2023). Indeed, long term recording of Gad2^{Fgf13 KO} mice (data not shown) confirmed that multiple spontaneous seizures occur in the knockouts prior to death in the home cage.

While our data provide a clear connection between ablation of Fgf13 in inhibitory neurons and seizure susceptibility, we find that Fgf13 ablation in excitatory neurons does not increase seizure susceptibility. Indeed, complete neuronal knockout with Nestin-Cre conferred a relative increased survival compared to the interneuron specific knockout with Gad2-Cre. We speculate that this relative increased survival in the Nestin^{Fgf13 KO} mice could be technical, due to less efficient targeting of interneurons by Nestin-Cre (Liang, Hippenmeyer et al. 2012), but it may also be biological if Nestin-Cre targeting of both excitatory and inhibitory neurons is comparatively neuroprotective because of simultaneous loss of both excitation and inhibition and consequent compensation for the loss of inhibition. The previous observation that a global Fgf13 heterozygous mouse line survived with a normal life span (Puranam, He et al. 2015) could support the interpretation that deletion from other cell types is comparatively neuroprotective. Moreover, our observations that our Emx1^{Fgf13 KO} mice do not suffer seizures is consistent with an earlier study of Emx1^{Fgf13 KO} mice, in which seizures were not reported (Wu, Yang et al. 2012). Previous studies suggested that FGF13-S, the isoform most highly expressed in excitatory neurons, confers long-term inactivation (Venkatesan, Liu et al. 2014, Fry, Marra et al. 2021), and the reduction of long-term inactivation due to DEE-associated variants drives increased excitability as the mechanism for seizures (Fry, Marra et al. 2021). Our data confirm the ability of FGF13-S to impart long-term inactivation and that ablation of Fgf13 in excitatory neurons eliminates long-term inactivation, yet this mechanism does not likely contribute to seizure susceptibility. Rather, knockout of Fgf13 in central nervous system excitatory neurons appears to affect learning and memory (Wu, Yang et al. 2012), which we did not assess here. An important limitation of our knockout models, however, is that they cannot provide direct insight into how missense variants reported in patients contribute to seizures. Nevertheless, since our Emx1^{Fgf13 KO} mice show a loss of long-term inactivation in excitatory neurons—the proposed mechanism by which the missense variants drive seizures—our model provides new boundaries on how those missense variants act in excitatory neurons.

Further, other than long-term inactivation, data herein show that Fgf13 ablation led to relatively minor effects on neuronal voltage-gated Na⁺ currents in Emx1⁺ excitatory neurons compared to previous results from others and us (Venkatesan, Liu et al. 2014, Barbosa, Xiao et al. 2016, Pablo, Wang et al. 2016, Wang, Yang et al. 2021, Shen, Yue et al. 2022). Those neuronal studies investigated DRG neurons, or CNS neurons via RNAi-mediated knockdown of infusion of antibodies targeting the FGF13-S N-terminus, and not a cell-type specific knockout as we studied here, thus suggesting differences in the models studied. As the FGF13 DEEs result from a stable germ-line variants, the knockout model here (in contrast to knockdown approaches in cultured CNS neurons or acute infusion of antibodies) likely represents a more relevant disease model.

How does loss of FGF13 in inhibitory interneurons confer seizure susceptibility? Although knockout of Fgf13 in Gad2⁺ neurons decreased excitability and reduced overall inhibitory drive to pyramidal cells, knockout surprisingly did not affect Na_V currents in inhibitory neurons. This conclusion fits well with our previous report that the cytoplasmic C-terminal in Na_V1.1, the major Na_V channel expressed in inhibitory neurons, has a substitution of an amino acid that reduces FHF binding (Wang, Chung et al. 2012), thus rendering these Na_V1.1 channels—and thus Na_V current in inhibitory interneurons—poor targets for FHF regulation. Rather, we found that perturbed excitability in interneurons lacking Fgf13 results from reduced K⁺ currents. This fits with our demonstration in cardiomyocytes that loss of FGF13 similarly reduces repolarizing K_V currents (Wang, Tang et al. 2017). Moreover, these data build upon the growing recognition that FHFs exert effects beyond Na_V channel regulation—the focus of most FHF studies since FHFs were identified as capable of directly interacting with Na_V channel C-termini (Liu, Dib-Hajj et al. 2001). Other identified roles for FGF13, such as regulating microtubule stability (Wu, Yang et al. 2012), affecting ribosome biogenesis (Bublik, Bursac et al. 2017), or generating axoaxonic synapses in chandelier cells (Favuzzi, Deogracias et al. 2019) may also contribute, but we did not investigate those roles here. The mechanism(s) by which FGF13 affects K_V currents is not known—we have not detected direct interaction between FHFs and K_V channels—but we speculate that the identified role for FGF13 in stabilizing microtubules may contribute, as microtubules regulate trafficking of ion channels to the plasma membrane during channel biogenesis (Vacher, Mohapatra et al. 2008).

Although we did not test it directly, our data are consistent with a possible role for FGF13 in chandelier cell function. Chandelier cells are fast-spiking GABAergic interneurons that uniquely target the axon initial segment of pyramidal cells. Chandelier cells are found sparsely in the brain, but are highly branched, enabling contact on hundreds of neighboring pyramidal cells (Compans and Burrone 2023). Fgf13 has previously been identified as a key molecule in the development of chandelier cell axons (Favuzzi, Deogracias et al. 2019), but whether Fgf13 subsequently contributes to their function has not been reported. Chandelier cells originate from the MGE, alongside parvalbumin- and somatostatin-expressing interneurons (Gallo, Paul et al. 2020). As our Nkx2.1^{Fgf13 KO} mice target deletion of Fgf13 from all the above subtypes, our data suggest that FGF13 may regulate chandelier cell function in seizure generation. Although chandelier cells have been shown to depolarize pyramidal cells and therefore exert a pro-excitatory role in the cortex(Szabadics, Varga et al. 2006), we observe otherwise in our mouse model in which decreased interneuron excitability results in a pro-excitatory state.

Understanding the molecular mechanisms that drive the pathogenesis of Fgf13-related seizures will enhance our understanding of DEEs and epilepsy at large. Future work will reveal the mechanisms of FGF13 interaction with potassium channels or other molecules that enable interneuron repolarization and excitability.

Acknowledgements

Supported by T32 DA03980 and F31 DA053796 (SL) and R01 HL160089 (GSP). We thank Andrew S. Lee and Gülcan Akgül for critical reading of the manuscript, as well as Mattia Malvezzi and Maiko Matsui for thoughtful discussions.

Conflicts of Interest

GSP is a scientific advisory board member for Tevard Biosciences. None of the other authors report any conflicts.