Search tips
Search criteria 


Logo of springeropenLink to Publisher's site
Molecular Neurobiology
Mol Neurobiol. 2017; 54(4): 2562–2578.
Published online 2016 March 19. doi:  10.1007/s12035-016-9821-6
PMCID: PMC5390005

Kainic Acid Induces mTORC1-Dependent Expression of Elmo1 in Hippocampal Neurons


Epileptogenesis is a process triggered by initial environmental or genetic factors that result in epilepsy and may continue during disease progression. Important parts of this process include changes in transcriptome and the pathological rewiring of neuronal circuits that involves changes in neuronal morphology. Mammalian/mechanistic target of rapamycin (mTOR) is upregulated by proconvulsive drugs, e.g., kainic acid, and is needed for progression of epileptogenesis, but molecular aspects of its contribution are not fully understood. Since mTOR can modulate transcription, we tested if rapamycin, an mTOR complex 1 inhibitor, affects kainic acid-evoked transcriptome changes. Using microarray technology, we showed that rapamycin inhibits the kainic acid-induced expression of multiple functionally heterogeneous genes. We further focused on engulfment and cell motility 1 (Elmo1), which is a modulator of actin dynamics and therefore could contribute to pathological rewiring of neuronal circuits during epileptogenesis. We showed that prolonged overexpression of Elmo1 in cultured hippocampal neurons increased axonal growth, decreased dendritic spine density, and affected their shape. In conclusion, data presented herein show that increased mTORC1 activity in response to kainic acid has no global effect on gene expression. Instead, our findings suggest that mTORC1 inhibition may affect development of epilepsy, by modulating expression of specific subset of genes, including Elmo1, and point to a potential role for Elmo1 in morphological changes that accompany epileptogenesis.

Electronic supplementary material

The online version of this article (doi:10.1007/s12035-016-9821-6) contains supplementary material, which is available to authorized users.

Keywords: Epilepsy, Rapamycin, Gene expression, mTORC1, Elmo1


Epilepsy is a common chronic neurological disorder that is characterized by recurrent seizures that are unpredictable and sometimes progressively severe [1]. Epilepsy is triggered by various environmental and genetic factors [2, 3] that induce numerous molecular changes, including changes in gene expression, that drive epileptogenesis [4, 5]. An important part of epileptogenesis is the pathological rewiring of neuronal circuits that involves changes in neuronal morphology (e.g., dendritic spine rearrangement and axonal sprouting; [6, 7]).

Several lines of evidence suggest links between epileptogenesis and complex 1 of mammalian/mechanistic target of rapamycin (mTOR), a serine-threonine protein kinase [8, 9]. On one hand, status epilepticus induces mTOR activation [1013]. On the other hand, rapamycin, an mTOR inhibitor, has antiepileptogenic effects in kainic acid (KA)-induced and pilocarpine-induced models of epilepsy in animals [1315]. Among other cellular roles, mTOR complex 1 (mTORC1) is known to control the transcription of several genes [16]. Our previous studies found increased nuclear levels of phosphorylated mTOR in hippocampal and cortical neurons cultured in vitro and in the brain in vivo after application of KA [11]. This observation could suggest that mTOR contributes to epileptogenesis by regulating gene expression. To test this hypothesis, in the present study, we aimed to evaluate effects of rapamycin on KA-evoked transcriptome changes in organotypic hippocampal slices using a microarray technology. The analysis revealed that mTORC1 is not a major driving force behind transcriptome changes induced by KA. Nevertheless, we found effects of rapamycin on the KA-induced expression of multiple functionally heterogeneous genes. One of them was engulfment and cell motility 1 (Elmo1), which duration of KA-induced expression was inhibited by rapamycin.

Elmo1, in complex with RhoG and Dock180, induces the activation of small GTPase Rac1 [17], a major regulator of actin dynamics [18]. Reorganized F-actin networks have been postulated to lead to the long-term stabilization of synaptic changes and consolidation of enhanced neuronal activity. Thus, alterations in F-actin network may be related to the aberrant hyperexcitability that is observed in epilepsy [19]. Rac1 and RhoA were significantly upregulated in the pentylenetetrazole kindling model and play a role in aberrant mossy fiber sprouting [20]. Links between Rac and epilepsy were further revealed by the impairment of hippocampal circuitry and epileptic phenotype of Rac1/Rac3 double-knockout mice [21]. Nonetheless, however, the role of Rho-family small GTPases and actin reorganization in epilepsy is poorly understood and the role of Elmo1 in epilepsy has not yet been elucidated. Thus, in the second part of this study, we investigated in more details effects of prolonged overexpression of Elmo1 in cultured hippocampal neurons and showed increased axonal growth, decreased dendritic spine density, and affected their shape.

Materials and Methods

Antibodies and Reagents

The antibodies that were used in the study are listed in Table Table1.1. The following reagents were used for pharmacological treatments: dimethylsulfoxide (DMSO; Sigma-Aldrich, St. Louis, MO, USA), rapamycin (R; LC Laboratories, Woburn, MA, USA), and kainic acid (KA, Tocris Bioscience, Ellisville, MO, USA). Hoechst 33342 was purchased from Life Technologies (Carlsbad, CA, USA).

Table 1
Antibodies used in the study

DNA Constructs

The mammalian expression plasmids β-actin-green fluorescent protein (GFP) and pSuper have been described previously [22, 23]. β-Actin-tdTomato plasmid, which encodes tdTomato under control of the β-actin promoter, was obtained by subcloning the tdTomato coding sequence using EcoRI/BamHI [24] to modified β-actin-16pl [25]. β-Actin-Elmo1-GFP was obtained by subcloning the rat Elmo1 coding sequence to EcoRI/SalI sites of β-actin-GFP. The coding sequence of Elmo1 was obtained from rat neuronal complementary DNA (cDNA) by polymerase chain reaction (PCR) using the following primers: 5′-GAGAATTCGTAATGCAGGTGGTGAAG-3′ and 5′-TGGTCGACTCAGTTACAGTCATAAACA-3′. pSuper-sh#Elmo1 was obtained by subcloning the previously described Elmo1 short hairpin RNA (shRNA) coding sequence [26] to pSuper.

Organotypic Hippocampal Slices

Hippocampal slice cultures were prepared based on the method described by Stoppini et al. [27] and in conformity with institutional guidelines of the First Local Ethics Committee in Warsaw (decision no. 861/2007), which are in compliance with the European Community Council Directive (86/609/EEC). Briefly, 8- to 10-day-old Wistar rat pups were decapitated without anesthesia and the hippocampi were dissected. Sections (400 μm) were prepared using a McIlwain tissue chopper (Ted Pella, Redding, CA, USA) and separated under ice-cold Gey’s balanced salt solution (Sigma-Aldrich; supplemented with 5 mg/ml glucose and 1 % penicillin/streptomycin). Slices were plated on semiporous membranes (four per membrane; Millipore, Darmstadt, Germany) and maintained at 37 °C in 5 % CO2 in Minimum Essential Medium (MEM) supplemented with Earle’s salts (MP Biomedicals, Santa Ana, CA, USA) and 25 % Hanks’ balanced salt solution (HBSS; MP Biomedicals), 25 % heat-inactivated horse serum (Sigma-Aldrich), 5 mg/ml glucose, 1 mM glutamine, and 1 % penicillin/streptomycin (all from Sigma-Aldrich). The maintenance media was changed every 3–4 days. For pharmacological treatments, slices on day 5 in vitro (DIV5) were treated either with vehicle (DMSO) or 10 μM KA (Fig. 1a). To inhibit mTOR activity, 20 nM rapamycin was added to slices either alone or in combination with KA (Fig. 1a). Rapamycin was added 2 h prior to KA. Slices were collected 0.5, 2, 6, and 24 h after KA treatment (Fig. 1a). For the analysis of aberrant axonal sprouting, DIV10 slices were treated with 6 μM KA for 48 h. Rapamycin was added 2 h prior to KA and present during KA treatment. The medium was then changed to maintenance medium, and slices were cultured until DIV26.

Fig. 1
In vitro model system to study molecular and cellular responses to kainic acid. a Scheme of rat organotypic hippocampal slice treatments with kainic acid (KA) and rapamycin (R). b Expression of c-Fos mRNA after KA treatment analyzed by qRT-PCR. C control, ...

Animals and Pharmacological Treatment

For the pharmacological experiments, 3-month-old male Wistar rats were used and described procedures were conducted in conformity with the institutional guidelines of the First Local Ethics Committee in Warsaw (decision no. 76/2010), which are in compliance with the European Community Council Directive (86/609/EEC). Tissue for messenger RNA (mRNA) analysis was collected during experiments described by Macias et al. [11]. Briefly, the animals were divided into four groups: vehicle, KA, rapamycin, and rapamycin+KA. Rapamycin was initially dissolved in 100 % ethanol for long-term storage. Prior to the injection, rapamycin was diluted in a vehicle solution that contained 5 % Tween 80 and 5 % PEG 400 (low-molecular-weight grade of polyethylene glycol; Sigma) and injected intraperitoneally (i.p.; 10 mg/kg) three times per week for 4 weeks. A control group of rats was injected with vehicle solution (5 % Tween 80, 5 % PEG 400, and 4 % ethanol). KA (10 mg/kg) was delivered by i.p. injection. In the rapamycin+KA group, KA was injected 48 h after the last dose of rapamycin. KA-injected animals were observed, and their behavior was digitally recorded. Severity of seizures was assessed according to a modified Racine’s scale [28]. Only the animals that displayed three episodes of generalized seizures (stage 3) were further analyzed. The rats were sacrificed 2 h following KA injection. Next, cortices and hippocampi were dissected from the brains and stored in RNAlater (Life Technology, Carlsbad, CA, USA) in −80 °C until use.

Primary Hippocampal and Cortical Neuron Cultures, Transfection, and Pharmacological Treatment

Animals that were used to obtain neurons for cell culture were sacrificed according to the protocol approved by the First Ethical Committee in Warsaw, Poland (decision no. 76/2010). Primary hippocampal and cortical cultures were prepared from embryonic day 19 (E19) rat brains as described previously [29]. Cells were plated on coverslips coated with poly-L-lysine (37.5 μg/ml, Sigma-Aldrich) and laminin (2.5 μg/ml, Roche, Basel, Switzerland) at a density of 500 cells/mm2 (hippocampal) or precoated BioCoat plastic plates (BD Biosciences Discovery Labware, San Jose, CA, USA) at a density of 1250/mm2 (cortical). Neuronal cultures were grown in Neurobasal medium (Life Technologies) supplemented with B27 (Life Technologies), 0.5 mM glutamine, 12.5 μM glutamate, and penicillin/streptomycin mix (all from Sigma-Aldrich). For the morphology experiments on day in vitro (DIV) 1, 8, or 18 hippocampal cultures were transfected using Lipofectamine2000 (Life Technologies) for 3 days as described previously [30]. In the overexpression experiments, β-actin-GFP or β-actin-Elmo1-GFP was cotransfected with β-actin-tdTomato at a 3:1 ratio. To visualize dendritic protrusions, the cells were stained with GFP tags. To characterize anti-Elmo1 antibody, cortical cultures were transfected on DIV0 using an Amaxa Nucleofector II Device and Amaxa Rat Neuron Nucleofactor Kit (Lonza, Basel, Switzerland) according to a modification of the manufacturer’s protocol [31] with pSuper or pSuper-sh#Elmo1 and β-actin-GFP or β-actin-Elmo1-GFP. Four days later, the cells were lysed.

For pharmacological treatments on DIV14, cortical cultures were treated with either vehicle (DMSO, control) or 25 μM KA for 10 min. To inhibit mTOR activity, 20 nM rapamycin was added to the cultures either alone or in combination with KA. Cortical cultures were collected 4 and 24 h after KA treatment and then lysed in sodium dodecyl sulfate (SDS) sample buffer for Western blot analysis or RNAlater for reverse-transcription quantitative real-time polymerase chain reaction (qRT-PCR) analysis.

Immunofluorescent Labeling

For the immunofluorescent staining of overexpressed proteins, neurons were fixed with 4 % paraformaldehyde (PFA) that contained 4 % sucrose in phosphate-buffered saline (PBS) for 10 min at room temperature. After fixation, the cells were washed three times with PBS for 5 min at room temperature and incubated with primary antibodies in GDB buffer (0.2 % gelatin, 0.8 M NaCl, 0.5 % Triton X-100, and 30 mM phosphate buffer, pH 7.4) overnight at 4 °C. The cells were then washed three times with PBS for 10 min at room temperature. Secondary antibodies were applied in GDB for 1 h at room temperature and underwent three washes with PBS, 10 min each. Secondary antibodies that were conjugated to Alexa Fluor 488 were used for labeling.

For immunofluorescent staining, organotypic slices were fixed with 4 % PFA that contained 4 % sucrose in PBS for 24 h at 4 °C. The slices were then washed with PBS that contained 0.2 % Triton-X100 (PBS-T), blocked with 5 % normal donkey serum in PBS-T, and incubated overnight at 4 °C with antibodies described in Table Table1,1, diluted in 1 % normal donkey serum (Sigma-Aldrich) in PBS-T. Afterward, the slices were rinsed with PBS-T and labeled for 1 h at room temperature with the respective secondary antibodies conjugated to Alexa Fluor dyes diluted 1:500 in 1 % donkey normal serum in PBS-T. After several washes with PBS-T, the slices were mounted on glass slides, air-dried, and sealed with Vectashield with Hoechst 33342 Mounting Medium (Vector Laboratories, Peterborough, UK). Results of c-Fos IF (Fig. 1c) were obtained from two independent slice cultures (eight animals). Slices from each animal were exposed to all types of treatment. At least two slices per animal per condition were analyzed. Results of P-S6 IF (Fig. 1d) were obtained from two independent slice cultures (three slices/condition/preparation were analyzed).

Terminal Deoxynucleotidyl Transferase dUTP Nick End Labeling Assay

The terminal deoxynucleotidyl transferase dUTP nick end labeling (TUNEL) assay was performed using the In Situ Cell Death Detection Kit, TMR red (Roche Applied Science, Mannheim, Germany). Organotypic hippocampal slices were permeabilized for 2 min on ice with permeabilization solution (0.1 % Triton X-100 and 1 % sodium citrate) and incubated with labeling solution plus enzyme solution at 37 °C for 1 h. As a negative control, the enzyme solution was omitted. The slices were then washed three times with PBS-T and counterstained with Hoechst 33342 dye and anti-GFAP antibody as described above. TUNEL staining was performed on two independent slice cultures (eight animals). Slices from each animal were exposed to all types of treatment. At least two slices per animal per condition were analyzed.

Confocal Imaging and Analysis

Images of immunofluorescently or TUNEL-stained neurons were acquired using confocal microscopy. Confocal images were obtained with sequential acquisition settings at 1024 × 1024 pixel resolution using a Zeiss LSM 5 Exciter microscope equipped with Ar (488 and 514 nm), HeNe (543 and 633 nm), and diode (405 nm) lasers. The laser power and image acquisition settings were kept constant. Each image was a z-series of images, each averaged twice. The obtained stack was “flattened” into a single image using maximum projection.

Morphometric analysis of axon and dendrite length, the number ends of axons and dendrites, and density, width and length of dendritic protrusions (spines and filopodia) of neurons in dissociated in vitro cultures was performed using MetaMorph image analysis software (Universal Imaging Corporation, Downingtown, PA, USA). For the total axon length and axonal ends, the full axonal tree of each neuron was traced on images acquired at a ×10 objective (0.6 digital zoom). The number of dendrites and dendrite length were quantified on images that were acquired with a ×40 objective (0.7 digital zoom) as described previously [23]. Quantification of the density, width, and length of dendritic protrusions was performed on images acquired with a ×40 objective (×5 digital zoom). The density of protrusions was counted as the number of protrusions on the 10 μm dendrite and three dendritic segments of one neuron. The average length, protrusion width, and density per cell for each cell were calculated and used for further averaging. Twenty randomly chosen cells were examined for each experimental condition for each culture batch. Data were obtained from three (analysis of axons or dendrites) or two (analysis of dendritic protrusions) independent batches of neurons. For further classification of protrusions, the protrusions were divided arbitrarily into two classes: filopodia (head width  0.4 μm) and spines (head width > 0.4 μm). The densities of filopodia and spines were next calculated as their number on the 10 μm of dendrite and expressed as percentage of all counted protrusions. Comparison of the protrusions length/width ratio were done as described by Cymerman et al. [32], and data are presented as % cumulative change.

Tissue Collection, RNA Preparation, and Gene Expression Profiling

To isolate RNA from organotypic hippocampal slices, at the end of the experiments, slices were placed in RNAlater reagent (Life Technology) and stored at −80 °C until use. RNA was isolated using the RNeasy Mini Kit (Qiagen, Venlo, The Netherlands) according to the manufacturer’s protocol. The total RNA concentration was measured using a NanoDrop Spectrometer 2000 (Thermo Fisher Scientific, Waltham, MA, USA), and its quality was determined by chip-based capillary electrophoresis using an RNA 6000 Nano LabChip Kit and Agilent Bioanalyzer 2100 (Agilent, Palo Alto, CA, USA) according to the manufacturer’s instructions. RNA from three independent biological repeats was pooled to create a sample for each microarray (e.g., single sample from one biological repeat that consisted of eight slices, each from different newborn rats of the same litter). A starting amount of 800 ng high-quality (RNA integrity numbers 9.8–9.9) total RNA (equally pooled from three independent experiments) was used to generate cDNA and complementary RNA (cRNA) with the Illumina TotalPrep RNA Amplification Kit (Illumina, San Diego, CA, USA). The obtained cDNA served as a template for in vitro transcription with T7 RNA polymerase and biotin UTP to generate multiple copies of biotinylated cRNA. Each cRNA sample (1.5 μg) was hybridized overnight to a RatRef-12 BeadChip array (Illumina). The chips were then washed, dried, and scanned with the BeadArray Reader (Illumina). Three biological replicates were used per time point and 12 arrays per each treatment group; the number of control samples was doubled. The treatment group samples were equally distributed between array plates and hybridization batches. Raw microarray data were generated using BeadStudio 3.0 (Illumina).

Microarray Data Analysis

Microarray quality control was performed using the BeadArray R package. The following parameters were checked on all 60 arrays: number of outliers, number of beads, and percentage of detected probes. After background subtraction, the data were normalized using quantile normalization and then log2-transformed. The obtained signal was taken as the measure of mRNA abundance derived from the level of gene expression. Statistical analysis of the results was performed using two-way analysis of variance (ANOVA), with KA and time as factors, followed by Benjamini and Hochberg correction for multiple testing (percent FDR; [33]). The effects of rapamycin on KA-induced alterations in gene expression are presented as differences in fold changes. All of the statistical analyses were performed using R software [34]. Hierarchical clustering was performed with dChip software using the Euclidean distance and average linkage method. The functional annotation analysis tool DAVID 2008 was used to identify overrepresented ontologic groups among the gene expression patterns and group genes into functional classifications [35]. The identification of overrepresented transcription factor binding sites (TFBSs) was performed using the cREMaG database with default parameters [36].

Reverse-Transcription Quantitative Real-Time Polymerase Chain Reaction

RNA from organotypic hippocampal slices, hippocampi or cultured neurons was isolated with the RNeasy Protect Mini Kit (Qiagen). cDNA was prepared with High Capacity RNA-to-cDNA Master Mix (Life Technologies) according to the manufacturer’s protocol. qRT-PCR was performed with a 7900HT machine and TaqMan Array Fast Plates (Life Technologies) with the following TaqMan rat probes: Tubb6 (Rn01253666_m1), Bdnf (Rn01484924_m1), Elmo1 (Rn01528402_m1), Lrrfip2 (Rn01245379_m1), Npas4 (Rn00596522_m1), Nr4a3 (Rn00581189_m1), Abra (Rn00598518_m1), Adrb1 (Rn00824536_s1), Cdr2 (Rn01511457_m1), Vgf (Rn00578591_g1), Gprc5a (Rn01459296_m1), Gadd45g (Rn01435432_g1), Nfil3 (Rn01434874_s1), Scg2 (Rn01400686_g1), Egr4 (Rn00569509_g1), and c-Fos (Rn02396759_m1). Actb (Rn00667869_m1) or Gapdh (Rn99999916_s1) was used as an internal control. SDS 2.4 and RQ Manager 1.2.1 programs were used for data acquisition and preliminary analysis.

Preparation of Protein Extracts and Western Blot Analysis

For the biochemical studies, organotypic hippocampal slices or cortical cultures were collected and stored at −80 °C until use. Cortical cultures were lysed in SDS sample buffer. To extract proteins from slices, the slices were lysed in homogenization buffer (10 mM Tris, pH 7.6, 150 mM NaCl, 2 mM EDTA, and 0.3 % 3-[(3-cholamidopropyl)dimethylammonio]-1-propanesulfonate [CHAPS]) supplemented with protease (Roche, Indianapolis, IN, USA) and phosphatase inhibitors (Sigma-Aldrich) and centrifuged at 14,000×g for 30 min at 4 °C. The supernatants were collected, and the protein concentration in the obtained protein lysates was measured using the DC Protein Assay (Bio-Rad Laboratories, Hercules, CA, USA). The proteins from both types of experiments were then analyzed by Western blot. After protein electrotransfer, the membranes were blocked for 1 h at room temperature in 5 % nonfat dry milk in TBS-T (Tris-buffer saline, pH 7.6, with 0.1 % Tween 20) and incubated overnight at 4 °C with primary antibodies (see Table Table1).1). For enhanced chemiluminescent detection (ECL), the next day, the membranes were washed several times with TBS-T and incubated for 1 h with horseradish peroxidase (HRP)-conjugated secondary antibodies diluted in TBS-T that contained 5 % nonfat dry milk (see Table Table1).1). Finally, the membranes were washed with TBS-T, incubated for 1 min with ECL reagent, and immediately exposed to X-ray film (Sigma-Aldrich). Western blot analysis of levels of phosphorylated ribosomal protein S6 (P-S6; Ser235/236), mTOR, caspase-3, and cleaved caspase-3 in organotypic slices (Fig. 2a) was performed on protein lysates obtained from three independent slice culture preparations (eight slices/condition/culture). The quantification of Western blot bands (Fig. 4) was performed using MetaMorph image analysis software (Universal Imaging Corporation, Downingtown, PA, USA). Bands that corresponded to Elmo1 and α-tubulin were manually traced, and their average area was automatically determined. The results are presented as the ratio of the average area of the Elmo1 band to the average area of the α-tubulin band.

Fig. 2
Kainic acid induces mTOR activity and cell death in organotypic hippocampal slices. a Western blot analysis of phosphorylated ribosomal protein S6 (P-S6; Ser235/236), mTOR, caspase-3, and cleaved caspase-3 in protein lysates obtained from organotypic ...
Fig. 4
Kainic acid-induced Elmo1 expression is mTOR-dependent in cultured cortical neurons. a Results of qRT-PCR-based analysis of Elmo1 expression in cortical neurons cultured in vitro for 5 days and treated as indicated (C control, R rapamycin, KA ...

Timm’s Sulfate Silver Staining

To visualize aberrant axonal sprouting, Timm staining was used [37]. Slices still placed in culture inserts, were incubated for 10 min with 1 % sodium sulfide in 0.1 M phosphate buffer (PB), followed by the gentle addition of 0.3 % glutaraldehyde in PB [37] and incubation for another 5 min. The slices were then washed with PB and postfixed overnight at 4 °C with 70 % ethanol. The next day, the preparations were washed again with PB and incubated with development solution (50 % gum arabic solution, 0.5 M hydroquinone solution, 1.2 M citric acid, 0.8 M trisodium citrate, and 0.37 M silver lactate) for 30 min in the dark. After this step, the slices were washed with water, and Timm staining was fixed with 5 % thiosulfate for 12 min, followed by washing with water. The slices were then incubated with 70 % ethanol for 30 min, placed on gelatin-coated glass slides, dehydrated, cleared, and coverslipped. Timm’s staining was performed on two independent slice cultures (eight animals). Two to four slices per condition were analyzed.

Statistical Analysis

The data were obtained from at least three batches of pooled slices or cultured cells. The results were analyzed using Prism software (GraphPad, La Jolla, CA, USA). For qRT-PCR analysis of c-fos expression and validation of microarray data, performed in slices and in vivo, we used Kruskal-Wallis test without following multiple comparisons tests due to low n of observations. For comparison of qRT-PCR and Western blot results obtained with use of cortical neurons, we used one-way ANOVA followed by Sidak’s multiple comparisons test. The Mann–Whitney test was used for the statistical analysis when two groups were compared. The statistical analysis of the microarrays was described in relevant section above.


Neuronal Responses to Kainic Acid Are Mimicked in Hippocampal Organotypic Slices

A previous study indicated that KA-induced status epilepticus results in substantial changes in the transcriptome [38] and increases mTOR activity in adult animals [11]. Although mTOR regulates transcription [16], this specific aspect has not been previously studied in the context of proconvulsive drug actions. Thus, we investigated the effects of rapamycin on KA-induced changes in the transcriptome. We first established a simplified in vitro culture model that allowed the reduction of heterogeneity of animal responses to KA and excluded the necessity for prolonged and repetitive rapamycin injections. We used DIV5 organotypic hippocampal slices from newborn rats and tested their responses to KA and mTOR inhibition (Figs. 1 and and2).2). These preparations, similar to intact animals, responded to KA with robust and transient expression of c-Fos, an immediate early gene, at the mRNA and protein levels (Fig. 1b, c). c-Fos mRNA and protein expression reached a maximum at 2 h post-KA (Kruskal-Wallis test with no post hoc test due to low n of observations, p < 0.01 for 2 and 6 h) and returned to control levels at 24 h. We also tested our preparations for cell death, astrogliosis, and the sprouting of mossy fibers (i.e., long-term changes that are typically evoked by KA in vivo; [39]. Both TUNEL staining and the analysis of caspase-3 cleavage confirmed enhanced cell death in slices upon KA treatment (Figs. 1d and and2a).2a). The immunofluorescent GFAP and MAP2 staining of slices confirmed that KA primarily affected survival of cells positive for MAP2 but not GFAP (Fig. 1d, e). GFAP immunostaining also revealed astrogliosis. Neuronal death that is induced by KA in the CA3 region of the hippocampus induces granule cells in the dentate gyrus to search for new synaptic targets, usually dendrites of other DG survivors. The formation of such aberrant connections, called aberrant sprouting, is a hallmark of epileptogenesis [40]. Timm’s sulfate silver staining revealed that KA that was added to organotypic hippocampal cultures induced mossy fiber sprouting 16 days post-KA. Consistent with previous in vivo results [11], rapamycin prevented this anatomical rearrangement (Fig. 1e). We next evaluated whether KA induces mTORC1 activity by monitoring the phosphorylation of ribosomal protein S6 (P-S6) at Ser 235/236. Similar to previously published results in intact animals [11], KA increased the level of P-S6 in a rapamycin-dependent manner (Fig. 2a, b). These results indicate that processes typically triggered by KA in vivo, like c-Fos expression and mTOR pathway induction, cell death, astrogliosis, and axonal sprouting can be also induced in organotypic hippocampal slices in response to KA.

Gene Expression Profiling of Kainic Acid- and Rapamycin-Induced Transcriptional Changes

Genomic research strategies have recently transitioned from the search for unknown genes to the identification and evaluation of coordinated gene networks and transcriptional signatures. Thus, to identify the potential contribution of mTOR to KA-evoked changes in the transcriptome, we used Illumina whole-genome rat microarrays to analyze the time course of gene expression alterations following KA administration in the presence or absence of rapamycin. To analyze the dynamics of early, intermediate, and relatively late changes in mRNA abundance, the analysis was performed 0.5, 2, 6, and 24 h after drug administration (Fig. 1a). We identified 81 KA-responsive genes (two-way ANOVA, FDR < 1 %), which were divided into five major clusters (A–E; Fig. 3a, Supplementary Table 1, Online Resource 1). The clusters revealed diverse KA-induced and time-dependent patterns of upregulation (clusters B–E) and downregulation (cluster A) of gene expression. Assuming the coordinated transcriptional regulation of identified genes, we searched for the overrepresentation of transcription factor binding sites. We found the overrepresentation of transcription factor binding sites, for such transcription factors as SRF (e.g., Egr1, Egr2, and Npas4) and CREB1 (e.g., Ier2, Dusp1, and Fos) in the promoter regions of the regulated genes (TFBS fold > 4; p < 0.05). As we expected, expression of the majority of these genes, present mostly in cluster D, was previously reported as dependent on neuronal activity. We also identified few genes regulated by rapamycin alone, including Sphk1, Penk1, and LOC304131 (two-way ANOVA, FDR < 1 %; Supplementary Table 2 [Online Resource 2] and Supplementary Fig. 1 [Online Resource 3]). Rapamycin induced alterations in the KA-induced expression of genes from cluster C (0.5 h time point according to scheme of experiment), cluster B (0.5 h time point), and cluster E (2 h time point) (Supplementary Table 1, Online Resource 1). Specifically, these effects, although weak, were visible as the enhanced induction of several genes from cluster B at the 2 h time point and inhibition of the expression of genes from clusters C and E at 2, 6, or 24 h (Supplementary Table 1, Online Resource 1 and Supplementary Fig. 2, Online Resource 3). Based on this evidence, we concluded that mTORC1 inhibition has discrete rather than global impact on KA-evoked transcriptome changes.

Fig. 3
Hierarchical clustering of transcriptional alterations in response to KA in rat hippocampal slices and validation of selected gene expression changes. a Microarray results are shown as a heat map and include rat genes with genome-wide significance (two-way ...

Effects of mTORC1 Inhibition on Kainic Acid-Induced Expression of Selected Genes

Although global analysis of the microarray data did not point to a group of genes with common characteristics that are regulated by mTORC1 in response to KA, of the list of genes that were differentially expressed between the KA and rapamycin+KA groups, we selected candidate genes, expression of which was downregulated by rapamycin (Supplementary Fig. 2, Online Resource 3), for further validation. We validated microarray results by qRT-PCR using total RNA that was isolated from organotypic hippocampal slices (mRNA aliquots were collected in parallel for both analyses). Detailed inspection of the microarray results revealed several genes, the levels of which differed between the KA and rapamycin+KA groups (e.g., Tubb6, Bdnf, Elmo1, Lrrfip2, Npas4, Nr4a3, Abra, Cdr2, Vgf, Gprc5a, Nfil3, Scg2, and Egr4 [all from cluster E] and Gadd45g [cluster C]; Fig. 3a; Supplementary Table 1, Online Resource 1). The expression patterns of the majority of the analyzed genes were consistent with those that were revealed by the microarray analysis (Fig. 3b, Supplementary Fig. 3 [Online Resource 3]). We observed the impact of rapamycin on the effects of KA for Elmo1, Abra, Gprc5a, Nr4a3, Vgf, Tubb6, Gadd45g, and Npas4. In many cases, qRT-PCR is more sensitive than microarrays. Therefore, the effects of rapamycin were detected at additional time points (Fig. 3b, Supplementary Fig. 3A [Online Resource 3]). In the case of Elmo1, Abra, Gprc5a, Nr4a3, Vgf, Tubb6, and Gadd45g, we noted an impact of rapamycin on their KA-induced expression also at earlier time points. To further validate our observations, we analyzed by qRT-PCR expression of selected genes in hippocampi of rats 2 h post-KA. As shown in Fig. 3c and Supplementary Fig. 3B (Online Resource 3), expression of Elmo1, Abra, Gprc5a, Nr4a3, Vgf, Npas4, Tubb6, and Gadd45g substantially increased compared to control rats. At the same time, long-term rapamycin pretreatment (4 weeks; see [11] for detailed description of experiment and validation of rapamycin effectiveness as mRNA was obtained in course of experiments described there) considerably decreased KA-induced increases of Elmo1, Abra, Gprc5a, Vgf, and Gadd45g mRNA levels. Thus, we concluded that KA-induced mTORC1-dependent changes in the selected gene expression, identified by microarray approach, indeed occur, both in hippocampal slices cultured in vitro as well as in the brain in vivo.

Long-Lasting Increase in Elmo1 Expression Affects Neuronal Morphology

We next focused on Elmo1 (cluster E) because its upregulation by KA was long-lasting and efficiently blocked by rapamycin at 6 and 24 h. What is more, Elmo1 was described to regulate actin cytoskeleton during neuronal development [26, 41]. To verify that KA-triggered changes in Elmo1 expression translate into alterations at the protein level, we produced a new anti-Elmo1 antibody because none of those that are commercially available met our specificity criteria (e.g., all tested antibodies recognized several bands, none of which was affected by RNA interference; not shown). This newly generated antibody, which targets the C-terminus of Elmo1, recognizes overexpressed and endogenous proteins of proper size in cultured cortical neurons that are electroporated with β-actin-Elmo1-GFP (Supplementary Fig. 4, Online Resource 3). Moreover, the signal that corresponded to the endogenous signal weakened upon the transfection of neurons with a plasmid that encoded shRNA against Elmo1 mRNA (Supplementary Fig. 4, Online Resource 3). Using this antibody, we sought to confirm the increase in Elmo1 protein in response to KA in our slice preparations. However, because of the low amount of protein, we did not obtain statistically significant confirmation. Therefore, to ensure a sufficient amount of material for the biochemical analysis, we switched to in vitro cultured cortical neurons. We first confirmed that KA treatment in these cells increased Elmo1 mRNA levels in a rapamycin-dependent manner. As shown in Fig. 4a, Elmo1 expression increased 4 h post-KA and rapamycin significantly prevented the effects of KA on Elmo1 mRNA levels. Similar results were found for Elmo1 protein levels (Fig. 4b, c). Decrease of P-S6 levels additionally confirmed that rapamycin efficiently silenced mTOR signaling at the tested time points (Fig. 4b).

Elmo1 is known to regulate F-actin dynamics, which underlies physiological and pathological rearrangements of neuronal morphology during development [26, 41]. Thus, we evaluated effects of the prolonged elevated expression of Elmo1 on the morphology of hippocampal neurons cultured in vitro at different developmental stages. Specifically, we morphometrically analyzed axonal and dendritic arbors of developing neurons and dendritic protrusions (spines and filopodia) of mature ones. Changes in axonal arborization and the number and shape of dendritic protrusions were previously reported in aberrant neuronal plasticity that accompanies epileptogenesis. We cotransfected cultured neurons for 3 days with β-actin-Elmo1-GFP and β-actin-tdTomato (to highlight the morphology of transfected neurons) and analyzed their morphology. We used DIV1, −7 developing, and −18 mature neurons for the analysis of axons, dendrites, and dendritic protrusions, respectively. As shown in Fig. 5a–c, axon length and number of axonal ends significantly increased upon Elmo1-GFP overexpression. In contrast, increases in the levels of Elmo1 did not affect either number of dendritic tips or total dendritic length (Fig. 5d–f). In case of dendritic protrusions the morphometric analysis revealed that cells that were transfected with β-actin-Elmo1-GFP had a lower density of dendritic protrusions compared with controls, which were also in average significantly longer (Fig. 5g–i). We also observed, tendency for dendritic protrusions width decrease in Elmo1 overexpressing neurons, which did not however reach statistical significance (Fig. 5j). Analysis of length to width ratio [32] indeed confirmed substantial shift of protrusion morphology toward filopodia-like one (Fig. 5k). Indeed, close inspection of specific frequencies of filopodia and spines in Elmo1 overexpressing cells revealed significant increase and decrease in filopodia and spine numbers, respectively (Fig. 5l, m). This suggests that Elmo1 overexpression in mature neurons, as oppose to developing ones [26] leads to spine destabilization and elimination.

Fig. 5
Elmo1 overexpression in hippocampal neurons affects axonal growth and dendritic spine morphology and density. a Representative confocal images of hippocampal neurons transfected on DIV1 with a plasmid that encoded GFP or Elmo1-GFP and fixed 3 days ...


mTOR inhibition has been considered for antiepileptogenic therapy [42, 43]. Epileptogenesis has been established to be associated with long-term changes in gene expression. We used a simplified in vitro culture system to investigate whether rapamycin affects transcriptome changes that are evoked by KA. We found that processes typically triggered by KA in vivo, like c-Fos expression and mTOR pathway induction, cell death, astrogliosis, and axonal sprouting were also induced in organotypic hippocampal slices in response to KA. The microarray analysis revealed changes in the transcription profiles of several genes in response to KA. Rapamycin affected only some of those changes, for example by preventing Elmo1, Abra, Gprc5a, Nr4a3, Vgf, Tubb6, Gadd45g, and Npas4 expression upregulation, suggesting that mTORC1 is not massively affecting KA-evoked transcriptome changes. We further focused on Elmo1, a modulator of actin dynamics and found that Elmo1 overexpression in hippocampal neurons increased axonal arborization and decreased dendritic spine density.

Effects of Kainic Acid on Organotypic Cultures in the Context of In Vivo Data

In this work, we described a simplified in vitro model to study molecular changes that are induced by KA. Importantly, we showed that the essential hallmarks of in vivo epileptogenesis (e.g., the induction of c-Fos expression, astrogliosis, neuronal death, and aberrant axonal sprouting) were reproduced in organotypic hippocampal slices in response to KA. One issue that arose was the extent to which our gene profiling results are consistent with data from in vivo models. Multiple gene profiling studies have been conducted using animal models of epilepsy [44]. Differentially expressed genes have been reported in status epilepticus or poststatus epilepticus rodent models, e.g. application of KA [45, 46] and pilocarpine [47, 48], or electrical stimulation [49, 50]. Notably, despite the large amount of data that have already accumulated, a comparative meta-analysis is difficult to perform because of the different experimental designs and microarray platforms that have been used in previous studies. Our data overlap to a largest extent with those of Kuzniewska et al. [46], who performed gene profiling in response to intrahippocampus-administered KA. Among the overlapping genes were Elmo1, Gadd45g, Npas4, Egr4, Gprc5a, Scg2, Nr4a3, Egr1, and Zfp36. Also, other genes identified by us were previously reported in animal models of epilepsy, including c-Fos and c-Jun [51], Bdnf [52], Dusp1 [53], Arc [54], Penk1 [5557], Egr2 [58], Crem [59], and Id1 [60, 61]. Thus, we conclude that our simplified model recapitulates major molecular and cellular changes that are observed in in vivo models of epilepsy. Consistently, several genes, expression of which was induced by KA in rapamycin-dependent manner in organotypic hippocampal cultures were controlled in similar way in vivo (Fig. 3c).

Effects of Rapamycin on Kainic Acid-Induced Gene Expression

Several recent reports suggest that the mTOR pathway may be central to epileptogenesis and therefore could be a convenient therapeutic target [14, 62]. Rapamycin has antiepileptogenic effects (e.g. prevents aberrant mossy fiber sprouting, appearance of recurrent seizures) in models of epilepsy in animals [1215]. In the present study, we focused on the influence of rapamycin on mRNA expression profiles under basal conditions and in response to KA. Our major observation was that rapamycin influences the expression of a small subset of genes induced by KA, rather than globally counteracts changes induced in transcriptome by KA. This is consistent with multiple actions of rapamycin including decrease in protein synthesis and induction of autophagy, which both may contribute to epileptogenesis prevention [63, 64]. Still it raises a question, what is the molecular mechanism that underlies the effects of rapamycin on KA-driven gene expression and provides observed selectivity of rapamycin effects. Because gene profiling only reveals the amount of a transcript, one should consider the role of mTOR in either the regulation of transcription or mRNA stabilization. In nonneuronal cells, mTOR is known to regulate activity, cellular localization, and the level of several transcription factors [16], e.g., hypoxia-inducible factor 1α (HIF-1α), increased expression of which was reported in animal models of epilepsy [65, 66]. However, in our analysis, we did not identify TFBS for HIF-1α in promoters of KA-upregulated genes that were affected by rapamycin. However, several rapamycin-modulated genes (e.g., Elmo1, Gadd45g, and Npas4) were also identified in a recent transcriptome study by Kuzniewska et al. [46], as controlled by SRF in response to KA. Additionally, chronic rapamycin treatment in rats and SRF knockout in the mouse forebrain increased the susceptibility to seizures and their severity [11, 46]. One issue is the way in which mTOR influences SRF transcriptional activity. Although no potential mechanism has been described to date, the present results identified Abra (STARS) as a rapamycin-modulated gene. The Abra product activates SRF-dependent transcription, inducing the nuclear translocation of megakaryoblastic leukemia 1 (MKL1) or MKL2 [67]. Thus, rapamycin could theoretically specifically downregulate SRF-dependent transcription to regulate the cellular localization of MKLs.

An alternative explanation for the contribution of mTOR to KA-induced gene expression is its involvement in transcript stabilization. mTOR participates in this process in nonneuronal cells. For example, rapamycin decreases the steady-state level of collagen (COL1A1 and COL1A2) mRNA in fibroblasts and destabilizes inducible nitric oxide synthase mRNA in astrocytes and transient receptor potential melastatin 6 in renal tubular epithelial cells [6870]. Whether mTOR stabilizes transcripts that are induced by status epilepticus remains to be investigated.

Potential Contribution to Kainic Acid-Related Neuropathology at the Cellular Level

Our data suggest that mTOR inhibition modulates the KA-induced expression of a subset of genes, but unknown is whether it has a potential impact on epileptogenesis. Knowing their cellular functions, we hypothesize that rapamycin could modulate cell death and cytoskeleton rearrangements, which both contribute to epileptogenesis. For example, Gadd45g plays a role in neuronal apoptosis during KA-dependent status epilepticus [71]. Moreover, Abra [72, 73], Elmo1 [74, 75], and Nr4a3 [76] were previously implicated in apoptosis. In our model, however, we could not prove antiapoptotic effects of rapamycin (see Fig. 2 for lack of an effect of rapamycin on KA-induced cleavage of caspase-3). Therefore, one possibility is that rapamycin, although it affects the expression of potentially proapoptotic genes, is unable to prevent the first wave of excitotoxic cell death upon KA application. Among our candidates, the products of three genes (Tubb6, Abra, and Elmo1) are known to modulate the cytoskeleton. Tubb6 encodes β-tubulin, and dynamic microtubules contribute to axonal growth and spine shape changes [30, 77, 78]. Nonetheless, the particular functions of this β-tubulin isoform in the nervous system have not been described but its deletion may contribute to microcephaly (Jawad syndrome; [79]). Abra increases the actin polymerization of muscle cells [67], but its role in neurons has not been described. In theory, its lowered expression in response to rapamycin could prevent KA-induced neuronal changes in dendritic spine morphology or mossy fiber sprouting. Elmo1 is also a regulator of RhoA and Rac1. Via these small GTPases, it regulates actin dynamics. The potential contribution of Elmo1 to KA-induced changes is discussed below.

Potential Contribution of mTOR-Dependent Elmo1 Regulation to Pathology

In the present study, we identified Elmo1 as a gene whose expression is activated by KA and is modulated by rapamycin. Using cortical neuron cultures in vitro, we also demonstrated that changes in the amount of Elmo1 mRNA correlate well with changes in Elmo1 protein levels. Elmo1 is a regulator of RhoA and Rac1 and via these small GTPases Elmo1 regulates actin cytoskeleton. Elmo1 was shown to participate in neuronal apoptosis and neurite outgrowth [80]. Thus, in our in vitro model, the KA-induced expression of Elmo1 would be associated with reorganization of the cytoskeleton. Consequently, the downregulation of Elmo1 expression could explain the effects of rapamycin on KA-induced neuronal morphological changes, such as axon sprouting and spine shape rearrangements, which depend on the actin cytoskeleton. In the present study, we investigated effects of increased Elmo1 expression on morphology of developing and mature hippocampal neurons cultured in vitro. In case of developing cells, we reported that overexpression of Elmo1 induces axonal growth and arborization. This result corroborates potential role of Elmo1 in epilepsy-related sprouting but does not prove it because epilepsy-related sprouting occurs in mature cells. Unfortunately, for technical reasons, it was impossible to undoubtedly trace axons of mature neurons in our type of culture. Yet, our observation brings new information concerning Elmo1 and suggests that cellular availability of this protein may limit axonal growth during development. This result is somewhat contradictory with work of Franke et al. [41], who showed that RhoG/Elmo1/Dock180/Rac1 pathway restricts axonal branching of embryonic hippocampal neurons. Yet, Franke et al. [41] used mutant Elmo1, which can not bind Dock180 (Elmo1-D625) but did not study wild type Elmo1. Thus, one can speculate that Elmo1 possesses progrowth activity which is mitigated by Dock180. Alternatively, it is possible that Elmo1 acts also outside its canonical pathway during axonal growth, but in such case, the role of Rac1 and actin cytoskeleton cannot be readily claimed.

Another novel finding reported herein is that increased Elmo1 level in mature hippocampal neurons resulted in reduction of dendritic spine number as well as induced their shape change to filopodia-like one. Thus, increased Elmo1 expression in mature neurons, a model relevant to developmental stage for which we performed gene profiling experiments, seems to drive spine elimination. Notably, decreases in spine number have been reported in mouse brain 24 h post-KA [81]. It would be of interest to check if rapamycin prevents spine elimination induced by KA. In addition, our result suggests that Elmo1 plays different role in developing and mature neurons with regard to dendritic spines since Kim et al. [26], overexpressed Elmo1 in developing neurons at the advent of spinogenesis (DIV6) and reported slight increase in number of dendritic spines by DIV18.

In conclusion, data presented herein show that increased activity of mTORC1 in response to kainic acid is not affecting gene expression globally. However, our findings suggest that rapamycin, in addition to previously described activities, may indeed affect development of epilepsy, by modulating expression of specific subset of genes, including Elmo1 and point to a potential role for Elmo1 in morphological changes that accompany epileptogenesis.

Electronic supplementary material

Below is the link to the electronic supplementary material.

Online resource 1(119K, xls)

(XLS 119 kb)

Online resource 2(26K, xls)

(XLS 25 kb)

Online resource 3(408K, pdf)

(PDF 407 kb)


We thank Roger Tsien for tdTomato cDNA. We also would like to express our gratitude to Lukasz Swiech, Agata Gozdz, Maciej Lipko, Artur Czupryn, Alina Zielinska, and Monika Matuszczyk for help with the experiments and technical assistance; to Michal Stronkowski for help with statistical analysis of data and to Erwin van Vliet and Michal Hetman for comments on the manuscript. We thank Bozena Kaminska-Kaczmarek for providing access to the Agilent Bioanalyzer. This work was financed by the Ministry of Science and Higher Education (grant no. NN301-779040) and the Foundation for Polish Science PARENT-BRIDGE Programme to MB and the Polish-Norwegian Research Fund (grant no. PNRF-96-AI-1/07) and Polish National Science Centre OPUS grant (2012/05/B/NZ3/00429) to JJ. The work of MB, AT, and JJ was also partly financed by the European Community’s Seventh Framework Programme (FP7/2007-2013; EPISTOP, grant agreement no. 602391). JJ is a recipient of a “Mistrz” Professorial subsidy from the Foundation for Polish Science.

Author Contributions

JJ, MB, and RP designed the overall study and supervised the experiments. MB, MM, MU, and AS performed organotypic slice culture experiments and analyzed the data. MB, MK, and MP performed microarray experiments and analyzed the data. MB, MM, AS, and AT performed in vivo analysis of gene expression. MB, MF, MM, and AK performed experiments on dissociated neurons cultured in vitro and performed morphometric analysis. MB, MM, and MK prepared the figures. MB and JJ wrote the manuscript.

Compliance with Ethical Standards

Compliance with Ethical Standards

Conflict of Interest

The authors declare that they have no competing interests.


Electronic supplementary material

The online version of this article (doi:10.1007/s12035-016-9821-6) contains supplementary material, which is available to authorized users.

Contributor Information

Magdalena Blazejczyk, Phone: +48 22 597 07 55, lp.vog.bcmii@kyzcjezalbm.

Jacek Jaworski, Phone: +48 22 597 07 55, lp.vog.bcmii@iksrowaj.


1. Meng X-F, Yu J-T, Song J-H, et al. Role of the mTOR signaling pathway in epilepsy. J Neurol Sci. 2013;332:4–15. doi: 10.1016/j.jns.2013.05.029. [PubMed] [Cross Ref]
2. Kotloski RJ, Sutula TP. Environmental enrichment: evidence for an unexpected therapeutic influence. Exp Neurol. 2014;264C:121–126. [PubMed]
3. Olson HE, Poduri A, Pearl PL. Genetic forms of epilepsies and other paroxysmal disorders. Semin Neurol. 2014;34:266–279. doi: 10.1055/s-0034-1386765. [PMC free article] [PubMed] [Cross Ref]
4. Aronica E, Gorter JA. Gene expression profile in temporal lobe epilepsy. Neurosci Rev J Bringing Neurobiol Neurol Psychiatry. 2007;13:100–108. [PubMed]
5. Jung K-H, Chu K, Lee S-T, et al. Molecular alterations underlying epileptogenesis after prolonged febrile seizure and modulation by erythropoietin. Epilepsia. 2011;52:541–550. doi: 10.1111/j.1528-1167.2010.02916.x. [PubMed] [Cross Ref]
6. Bozzi Y, Casarosa S, Caleo M. Epilepsy as a neurodevelopmental disorder. Front Psychiatry. 2012;3:19. doi: 10.3389/fpsyt.2012.00019. [PMC free article] [PubMed] [Cross Ref]
7. Song M-Y, Tian F-F, Wang Y-Z, et al. Potential roles of the RGMa-FAK-Ras pathway in hippocampal mossy fiber sprouting in the pentylenetetrazole kindling model. Mol Med Rep. 2015;11:1738–1744. [PMC free article] [PubMed]
8. Curatolo P, D’Argenzio L, Cerminara C, Bombardieri R. Management of epilepsy in tuberous sclerosis complex. Expert Rev Neurother. 2008;8:457–467. doi: 10.1586/14737175.8.3.457. [PubMed] [Cross Ref]
9. Ryther RCC, Wong M. Mammalian target of rapamycin (mTOR) inhibition: potential for antiseizure, antiepileptogenic, and epileptostatic therapy. Curr Neurol Neurosci Rep. 2012;12:410–418. doi: 10.1007/s11910-012-0276-5. [PMC free article] [PubMed] [Cross Ref]
10. Buckmaster PS, Ingram EA, Wen X. Inhibition of the mammalian target of rapamycin signaling pathway suppresses dentate granule cell axon sprouting in a rodent model of temporal lobe epilepsy. J Neurosci Off J Soc Neurosci. 2009;29:8259–8269. doi: 10.1523/JNEUROSCI.4179-08.2009. [PMC free article] [PubMed] [Cross Ref]
11. Macias M, Blazejczyk M, Kazmierska P, et al. Spatiotemporal characterization of mTOR kinase activity following kainic acid induced status epilepticus and analysis of rat brain response to chronic rapamycin treatment. PLoS One. 2013;8 doi: 10.1371/journal.pone.0064455. [PMC free article] [PubMed] [Cross Ref]
12. van Vliet EA, Forte G, Holtman L, et al. Inhibition of mammalian target of rapamycin reduces epileptogenesis and blood–brain barrier leakage but not microglia activation. Epilepsia. 2012;53:1254–1263. doi: 10.1111/j.1528-1167.2012.03513.x. [PubMed] [Cross Ref]
13. Zeng L-H, Rensing NR, Wong M. The mammalian target of rapamycin signaling pathway mediates epileptogenesis in a model of temporal lobe epilepsy. J Neurosci Off J Soc Neurosci. 2009;29:6964–6972. doi: 10.1523/JNEUROSCI.0066-09.2009. [PMC free article] [PubMed] [Cross Ref]
14. Huang X, Zhang H, Yang J, et al. Pharmacological inhibition of the mammalian target of rapamycin pathway suppresses acquired epilepsy. Neurobiol Dis. 2010;40:193–199. doi: 10.1016/j.nbd.2010.05.024. [PMC free article] [PubMed] [Cross Ref]
15. Theilhaber J, Rakhade SN, Sudhalter J, et al. Gene expression profiling of a hypoxic seizure model of epilepsy suggests a role for mTOR and Wnt signaling in epileptogenesis. PLoS One. 2013;8 doi: 10.1371/journal.pone.0074428. [PMC free article] [PubMed] [Cross Ref]
16. Malik AR, Urbanska M, Macias M, et al. Beyond control of protein translation: what we have learned about the non-canonical regulation and function of mammalian target of rapamycin (mTOR) Biochim Biophys Acta BBA Proteins Proteomics. 2013;1834:1434–1448. doi: 10.1016/j.bbapap.2012.12.010. [PubMed] [Cross Ref]
17. Katoh H, Negishi M. RhoG activates Rac1 by direct interaction with the Dock180-binding protein Elmo. Nature. 2003;424:461–464. doi: 10.1038/nature01817. [PubMed] [Cross Ref]
18. Etienne-Manneville S, Hall A. Rho GTPases in cell biology. Nature. 2002;420:629–635. doi: 10.1038/nature01148. [PubMed] [Cross Ref]
19. Zhang Y-F, Li S-L, Xiong T-Q, et al. The rearrangement of filamentous actin in mossy fiber synapses in pentylenetetrazol-kindled C57BL/6 mice. Epilepsy Res. 2014;108:20–28. doi: 10.1016/j.eplepsyres.2013.10.019. [PubMed] [Cross Ref]
20. Dang J, Tian F, Li F, et al. Roles of Rho guanine nucleotide triphosphatases in hippocampal mossy fiber sprouting in the pentylenetetrazole kindling model. Clin Lab. 2014;60:175–184. doi: 10.7754/Clin.Lab.2013.130320. [PubMed] [Cross Ref]
21. Corbetta S, Gualdoni S, Ciceri G, et al. Essential role of Rac1 and Rac3 GTPases in neuronal development. FASEB J Off Publ Fed Am Soc Exp Biol. 2009;23:1347–1357. [PubMed]
22. Brummelkamp TR, Bernards R, Agami R. A system for stable expression of short interfering RNAs in mammalian cells. Science. 2002;296:550–553. doi: 10.1126/science.1068999. [PubMed] [Cross Ref]
23. Jaworski J, Spangler S, Seeburg DP, et al. Control of dendritic arborization by the phosphoinositide-3′-kinase-Akt-mammalian target of rapamycin pathway. J Neurosci Off J Soc Neurosci. 2005;25:11300–11312. doi: 10.1523/JNEUROSCI.2270-05.2005. [PubMed] [Cross Ref]
24. Shaner NC, Campbell RE, Steinbach PA, et al. Improved monomeric red, orange and yellow fluorescent proteins derived from Discosoma sp. red fluorescent protein. Nat Biotechnol. 2004;22:1567–1572. doi: 10.1038/nbt1037. [PubMed] [Cross Ref]
25. Kaech S, Ludin B, Matus A. Cytoskeletal plasticity in cells expressing neuronal microtubule-associated proteins. Neuron. 1996;17:1189–1199. doi: 10.1016/S0896-6273(00)80249-4. [PubMed] [Cross Ref]
26. Kim J-Y, Oh MH, Bernard LP, et al. The RhoG/ELMO1/Dock180 signaling module is required for spine morphogenesis in hippocampal neurons. J Biol Chem. 2011;286:37615–37624. doi: 10.1074/jbc.M111.268029. [PMC free article] [PubMed] [Cross Ref]
27. Stoppini L, Buchs PA, Muller D. A simple method for organotypic cultures of nervous tissue. J Neurosci Methods. 1991;37:173–182. doi: 10.1016/0165-0270(91)90128-M. [PubMed] [Cross Ref]
28. Hellier JL, Patrylo PR, Buckmaster PS, Dudek FE. Recurrent spontaneous motor seizures after repeated low-dose systemic treatment with kainate: assessment of a rat model of temporal lobe epilepsy. Epilepsy Res. 1998;31:73–84. doi: 10.1016/S0920-1211(98)00017-5. [PubMed] [Cross Ref]
29. Banker G, Goslin K. Developments in neuronal cell culture. Nature. 1988;336:185–186. doi: 10.1038/336185a0. [PubMed] [Cross Ref]
30. Jaworski J, Kapitein LC, Gouveia SM, et al. Dynamic microtubules regulate dendritic spine morphology and synaptic plasticity. Neuron. 2009;61:85–100. doi: 10.1016/j.neuron.2008.11.013. [PubMed] [Cross Ref]
31. Perycz M, Urbanska AS, Krawczyk PS, et al. Zipcode binding protein 1 regulates the development of dendritic arbors in hippocampal neurons. J Neurosci. 2011;31:5271–5285. doi: 10.1523/JNEUROSCI.2387-10.2011. [PubMed] [Cross Ref]
32. Cymerman IA, Gozdz A, Urbanska M, et al. Structural plasticity of dendritic spines requires GSK3α and GSK3β PLoS One. 2015;10 doi: 10.1371/journal.pone.0134018. [PMC free article] [PubMed] [Cross Ref]
33. Benjamini Y, Hochberg Y. Controlling the false discovery rate: a practical and powerful approach to multiple testing. J R Stat Soc Ser B Methodol. 1995;57:289–300.
34. Gentleman RC, Carey VJ, Bates DM, et al. Bioconductor: open software development for computational biology and bioinformatics. Genome Biol. 2004;5:R80. doi: 10.1186/gb-2004-5-10-r80. [PMC free article] [PubMed] [Cross Ref]
35. Huang DW, Sherman BT, Lempicki RA. Systematic and integrative analysis of large gene lists using DAVID bioinformatics resources. Nat Protoc. 2008;4:44–57. doi: 10.1038/nprot.2008.211. [PubMed] [Cross Ref]
36. Piechota M, Korostynski M, Przewlocki R. Identification of cis-regulatory elements in the mammalian genome: the cREMaG database. PLoS ONE. 2010;5 doi: 10.1371/journal.pone.0012465. [PMC free article] [PubMed] [Cross Ref]
37. Danscher G. Histochemical demonstration of heavy metals. A revised version of the sulphide silver method suitable for both light and electronmicroscopy. Histochemistry. 1981;71:1–16. doi: 10.1007/BF00592566. [PubMed] [Cross Ref]
38. Laurén HB, Lopez-Picon FR, Brandt AM, et al. Transcriptome analysis of the hippocampal CA1 pyramidal cell region after kainic acid-induced status epilepticus in juvenile rats. PLoS One. 2010;5 doi: 10.1371/journal.pone.0010733. [PMC free article] [PubMed] [Cross Ref]
39. Dudek FE, Clark S, Williams PA, Grabenstatter HL. Chapter 34 - kainate-induced status epilepticus: a chronic model of accuired epilepsy. In: Moshé APASL, editor. Models seizures epilepsy. Burlington: Academic; 2006. pp. 415–432.
40. Cavazos J, Jones S, Cross D. Sprouting and synaptic reorganization in the subiculum and CA1 region of the hippocampus in acute and chronic models of partial-onset epilepsy. Neuroscience. 2004;126:677–688. doi: 10.1016/j.neuroscience.2004.04.014. [PMC free article] [PubMed] [Cross Ref]
41. Franke K, Otto W, Johannes S, et al. miR-124-regulated RhoG reduces neuronal process complexity via ELMO/Dock180/Rac1 and Cdc42 signalling. EMBO J. 2012;31:2908–2921. doi: 10.1038/emboj.2012.130. [PubMed] [Cross Ref]
42. Galanopoulou AS, Gorter JA, Cepeda C. Finding a better drug for epilepsy: the mTOR pathway as an antiepileptogenic target. Epilepsia. 2012;53:1119–1130. doi: 10.1111/j.1528-1167.2012.03506.x. [PMC free article] [PubMed] [Cross Ref]
43. Curatolo P, Moavero R. mTOR inhibitors as a new therapeutic option for epilepsy. Expert Rev Neurother. 2013;13:627–638. doi: 10.1586/ern.13.49. [PubMed] [Cross Ref]
44. Wang YY, Smith P, Murphy M, Cook M. Global expression profiling in epileptogenesis: does it add to the confusion? Brain Pathol Zurich Switz. 2010;20:1–16. doi: 10.1111/j.1750-3639.2008.00254.x. [PMC free article] [PubMed] [Cross Ref]
45. Hunsberger JG, Bennett AH, Selvanayagam E, et al. Gene profiling the response to kainic acid induced seizures. Brain Res Mol Brain Res. 2005;141:95–112. doi: 10.1016/j.molbrainres.2005.08.005. [PubMed] [Cross Ref]
46. Kuzniewska B, Nader K, Dabrowski M, et al. Adult deletion of SRF increases epileptogenesis and decreases activity-induced gene expression. Mol Neurobiol. 2015 [PMC free article] [PubMed]
47. Becker AJ, Chen J, Zien A, et al. Correlated stage- and subfield-associated hippocampal gene expression patterns in experimental and human temporal lobe epilepsy. Eur J Neurosci. 2003;18:2792–2802. doi: 10.1111/j.1460-9568.2003.02993.x. [PubMed] [Cross Ref]
48. Elliott RC, Miles MF, Lowenstein DH. Overlapping microarray profiles of dentate gyrus gene expression during development- and epilepsy-associated neurogenesis and axon outgrowth. J Neurosci. 2003;23:2218–2227. [PubMed]
49. Gorter JA, van Vliet EA, Aronica E, et al. Potential new antiepileptogenic targets indicated by microarray analysis in a rat model for temporal lobe epilepsy. J Neurosci. 2006;26:11083–11110. doi: 10.1523/JNEUROSCI.2766-06.2006. [PubMed] [Cross Ref]
50. Lukasiuk K, Kontula L, Pitkänen A. cDNA profiling of epileptogenesis in the rat brain. Eur J Neurosci. 2003;17:271–279. doi: 10.1046/j.1460-9568.2003.02461.x. [PubMed] [Cross Ref]
51. Kaminska B, Filipkowski RK, Zurkowska G, et al. Dynamic changes in the composition of the AP-1 transcription factor DNA-binding activity in rat brain following kainate-induced seizures and cell death. Eur J Neurosci. 1994;6:1558–1566. doi: 10.1111/j.1460-9568.1994.tb00546.x. [PubMed] [Cross Ref]
52. Dugich-Djordjevic MM, Tocco G, Willoughby DA, et al. BDNF mRNA expression in the developing rat brain following kainic acid-induced seizure activity. Neuron. 1992;8:1127–1138. doi: 10.1016/0896-6273(92)90133-X. [PubMed] [Cross Ref]
53. Boschert U, Dickinson R, Muda M, et al. Regulated expression of dual specificity protein phosphatases in rat brain. Neuroreport. 1998;9:4081–4086. doi: 10.1097/00001756-199812210-00014. [PubMed] [Cross Ref]
54. Toyoda T, Nomura H, Hashikawa K, et al. Persistent neural activity regulates Arc/Arg3.1 transcription in the dentate gyrus. J Neurosci Res. 2010;88:3060–3066. doi: 10.1002/jnr.22471. [PubMed] [Cross Ref]
55. Bing G, Wilson B, Hudson P, et al. A single dose of kainic acid elevates the levels of enkephalins and activator protein-1 transcription factors in the hippocampus for up to 1 year. Proc Natl Acad Sci U S A. 1997;94:9422–9427. doi: 10.1073/pnas.94.17.9422. [PubMed] [Cross Ref]
56. Lason W, Przewlocka B, Przewlocki R. The effects of excitatory amino acids on proenkephalin and prodynorphin mRNA levels in the hippocampal dentate gyrus of the rat; an in situ hybridization study. Brain Res Mol Brain Res. 1992;12:243–247. doi: 10.1016/0169-328X(92)90090-X. [PubMed] [Cross Ref]
57. Przewlocki R, Kaminska B, Lukasiuk K, et al. Seizure related changes in the regulation of opioid genes and transcription factors in the dentate gyrus of rat hippocampus. Neuroscience. 1995;68:73–81. doi: 10.1016/0306-4522(95)00144-8. [PubMed] [Cross Ref]
58. Honkaniemi J, Sharp FR. Prolonged expression of zinc finger immediate-early gene mRNAs and decreased protein synthesis following kainic acid induced seizures. Eur J Neurosci. 1999;11:10–17. doi: 10.1046/j.1460-9568.1999.00401.x. [PubMed] [Cross Ref]
59. Xu Y, Yu S, Shu Q, et al. Upregulation of CREM-1 relates to retinal ganglion cells apoptosis after light-induced damage in vivo. J Mol Neurosci. 2014;52:331–338. doi: 10.1007/s12031-013-0153-y. [PubMed] [Cross Ref]
60. Aronica E, Vandeputte DA, van Vliet EA, et al. Expression of Id proteins increases in astrocytes in the hippocampus of epileptic rats. Neuroreport. 2001;12:2461–2465. doi: 10.1097/00001756-200108080-00035. [PubMed] [Cross Ref]
61. Passiatore G, Gentilella A, Rom S, et al. Induction of Id-1 by FGF-2 involves activity of EGR-1 and sensitizes neuroblastoma cells to cell death. J Cell Physiol. 2011;226:1763–1770. doi: 10.1002/jcp.22505. [PMC free article] [PubMed] [Cross Ref]
62. Wong M. Rapamycin for treatment of epilepsy: antiseizure, antiepileptogenic, both, or neither? Epilepsy Curr Am Epilepsy Soc. 2011;11:66–68. doi: 10.5698/1535-7511-11.2.66. [PMC free article] [PubMed] [Cross Ref]
63. Jones LS, Grooms SY, Lapadula DM, Lewis DV. Protein synthesis inhibition blocks maintenance but not induction of epileptogenesis in hippocampal slice. Brain Res. 1992;599:338–344. doi: 10.1016/0006-8993(92)90410-B. [PubMed] [Cross Ref]
64. McMahon J, Huang X, Yang J, et al. Impaired autophagy in neurons after disinhibition of mammalian target of rapamycin and its contribution to epileptogenesis. J Neurosci Off J Soc Neurosci. 2012;32:15704–15714. doi: 10.1523/JNEUROSCI.2392-12.2012. [PMC free article] [PubMed] [Cross Ref]
65. Li J, Jiang G, Chen Y, et al. Altered expression of hypoxia-Inducible factor-1α participates in the epileptogenesis in animal models. Synapse. 2014;68:402–409. doi: 10.1002/syn.21745. [PubMed] [Cross Ref]
66. Long Q, Fan C, Kai W, et al. Hypoxia inducible factor-1α expression is associated with hippocampal apoptosis during epileptogenesis. Brain Res. 2014;1590:20–30. doi: 10.1016/j.brainres.2014.09.028. [PubMed] [Cross Ref]
67. Wallace MA, Russell AP. Striated muscle activator of Rho signaling is required for myotube survival but does not influence basal protein synthesis or degradation. Am J Physiol Cell Physiol. 2013;305:C414–C426. doi: 10.1152/ajpcell.00421.2012. [PubMed] [Cross Ref]
68. Ikari A, Sanada A, Sawada H, et al. Decrease in transient receptor potential melastatin 6 mRNA stability caused by rapamycin in renal tubular epithelial cells. Biochim Biophys Acta. 2011;1808:1502–1508. doi: 10.1016/j.bbamem.2010.11.006. [PubMed] [Cross Ref]
69. Lisi L, Navarra P, Feinstein DL, Dello Russo C. The mTOR kinase inhibitor rapamycin decreases iNOS mRNA stability in astrocytes. J Neuroinflammation. 2011;8:1. doi: 10.1186/1742-2094-8-1. [PMC free article] [PubMed] [Cross Ref]
70. Shegogue D, Trojanowska M. Mammalian target of rapamycin positively regulates collagen type I production via a phosphatidylinositol 3-kinase-independent pathway. J Biol Chem. 2004;279:23166–23175. doi: 10.1074/jbc.M401238200. [PubMed] [Cross Ref]
71. Henshall DC, Sinclair J, Simon RP. Relationship between seizure-induced transcription of the DNA damage-inducible gene GADD45, DNA fragmentation, and neuronal death in focally evoked limbic epilepsy. J Neurochem. 1999;73:1573–1583. doi: 10.1046/j.1471-4159.1999.0731573.x. [PubMed] [Cross Ref]
72. Koekemoer AL, Chong NW, Goodall AH, Samani NJ. Myocyte stress 1 plays an important role in cellular hypertrophy and protection against apoptosis. FEBS Lett. 2009;583:2964–2967. doi: 10.1016/j.febslet.2009.08.011. [PubMed] [Cross Ref]
73. Kuwahara K, Pipes GCT, McAnally J, et al. Modulation of adverse cardiac remodeling by STARS, a mediator of MEF2 signaling and SRF activity. J Clin Invest. 2007;117:1324–1334. doi: 10.1172/JCI31240. [PubMed] [Cross Ref]
74. deBakker CD, Haney LB, Kinchen JM, et al. Phagocytosis of apoptotic cells is regulated by a UNC-73/TRIO-MIG-2/RhoG signaling module and armadillo repeats of CED-12/ELMO. Curr Biol. 2004;14:2208–2216. doi: 10.1016/j.cub.2004.12.029. [PubMed] [Cross Ref]
75. Schäker K, Bartsch S, Patry C, et al. The bipartite rac1 Guanine nucleotide exchange factor engulfment and cell motility 1/dedicator of cytokinesis 180 (elmo1/dock180) protects endothelial cells from apoptosis in blood vessel development. J Biol Chem. 2015;290:6408–6418. doi: 10.1074/jbc.M114.633701. [PMC free article] [PubMed] [Cross Ref]
76. Mullican SE, Zhang S, Konopleva M, et al. Abrogation of nuclear receptors Nr4a3 and Nr4a1 leads to development of acute myeloid leukemia. Nat Med. 2007;13:730–735. doi: 10.1038/nm1579. [PubMed] [Cross Ref]
77. Jaworski J, Hoogenraad CC, Akhmanova A. Microtubule plus-end tracking proteins in differentiated mammalian cells. Int J Biochem Cell Biol. 2008;40:619–637. doi: 10.1016/j.biocel.2007.10.015. [PubMed] [Cross Ref]
78. Kapitein LC, Yau KW, Gouveia SM, et al. NMDA receptor activation suppresses microtubule growth and spine entry. J Neurosci. 2011;31:8194–8209. doi: 10.1523/JNEUROSCI.6215-10.2011. [PubMed] [Cross Ref]
79. Hassan MJ, Chishti MS, Jamal SM, et al. A syndromic form of autosomal recessive congenital microcephaly (Jawad syndrome) maps to chromosome 18p11.22-q11.2. Hum Genet. 2008;123:77–82. doi: 10.1007/s00439-007-0452-x. [PubMed] [Cross Ref]
80. Shi L. Dock protein family in brain development and neurological disease. Commun Integr Biol. 2013 [PMC free article] [PubMed]
81. Wilczynski GM, Konopacki FA, Wilczek E, et al. Important role of matrix metalloproteinase 9 in epileptogenesis. J Cell Biol. 2008;180:1021–1035. doi: 10.1083/jcb.200708213. [PMC free article] [PubMed] [Cross Ref]

Articles from Springer Open Choice are provided here courtesy of Springer