Molecular Neurobiology

, Volume 55, Issue 2, pp 1795–1813 | Cite as

Homozygous Expression of Mutant ELOVL4 Leads to Seizures and Death in a Novel Animal Model of Very Long-Chain Fatty Acid Deficiency

  • Blake R. Hopiavuori
  • Ferenc DeákEmail author
  • Joseph L. Wilkerson
  • Richard S. Brush
  • Nicole A. Rocha-Hopiavuori
  • Austin R. Hopiavuori
  • Kathryn G. Ozan
  • Michael T. Sullivan
  • Jonathan D. Wren
  • Constantin Georgescu
  • Luke Szweda
  • Vibhudutta Awasthi
  • Rheal Towner
  • David M. Sherry
  • Robert E. AndersonEmail author
  • Martin-Paul AgbagaEmail author
Open Access


Lipids are essential components of the nervous system. However, the functions of very long-chain fatty acids (VLC-FA; ≥ 28 carbons) in the brain are unknown. The enzyme ELOngation of Very Long-chain fatty acids-4 (ELOVL4) catalyzes the rate-limiting step in the biosynthesis of VLC-FA (Agbaga et al., Proc Natl Acad Sci USA 105(35): 12843–12848, 2008; Logan et al., J Lipid Res 55(4): 698–708, 2014), which we identified in the brain as saturated fatty acids (VLC-SFA). Homozygous mutations in ELOVL4 cause severe neuropathology in humans (Ozaki et al., JAMA Neurol 72(7): 797–805, 2015; Mir et al., BMC Med Genet 15: 25, 2014; Cadieux-Dion et al., JAMA Neurol 71(4): 470–475, 2014; Bourassa et al., JAMA Neurol 72(8): 942–943, 2015; Aldahmesh et al., Am J Hum Genet 89(6): 745–750, 2011) and are post-natal lethal in mice (Cameron et al., Int J Biol Sci 3(2): 111–119, 2007; Li et al., Int J Biol Sci 3(2): 120–128, 2007; McMahon et al., Molecular Vision 13: 258–272, 2007; Vasireddy et al., Hum Mol Genet 16(5): 471–482, 2007) from dehydration due to loss of VLC-SFA that comprise the skin permeability barrier. Double transgenic mice with homozygous knock-in of the Stargardt-like macular dystrophy (STDG3; 797-801_AACTT) mutation of Elovl4 with skin-specific rescue of wild-type Elovl4 expression (S + Elovl4 mut/mut mice) develop seizures by P19 and die by P21. Electrophysiological analyses of hippocampal slices showed aberrant epileptogenic activity in S + Elovl4 mut/mut mice. FM1-43 dye release studies showed that synapses made by cultured hippocampal neurons from S + Elovl4 mut/mut mice exhibited accelerated synaptic release kinetics. Supplementation of VLC-SFA to cultured hippocampal neurons from mutant mice rescued defective synaptic release to wild-type rates. Together, these studies establish a critical, novel role for ELOVL4 and its VLC-SFA products in regulating synaptic release kinetics and epileptogenesis. Future studies aimed at understanding the molecular mechanisms by which VLC-SFA regulate synaptic function may provide new targets for improved seizure therapies.


ELOVL4 Very long-chain saturated fatty acids Synaptic vesicle fusion kinetics Synaptic dysregulation Seizure Brain lipids 


Heterozygous inheritance of four different mutations in exon 6 of the gene encoding the enzyme ELOngation of Very Long-chain fatty acids-4 (ELOVL4) develop a form of macular degeneration known as Stargardt-like macular dystrophy (STGD3) [1, 2, 3]. Our group discovered that ELOVL4 is a fatty acid elongase responsible for catalyzing the rate-limiting condensation reaction in the biosynthesis of very long-chain fatty acids (VLC-FA; ≥C28) [4]. We further showed that one of the STGD3 causing mutations, a 5-bp deletion in the exon 6 of ELOVL4 (797-801_AACTT), results in an enzymatically inactive mutant protein [5]. VLC-FA are present as components of more complex lipid molecules with tissue-specific distribution. ELOVL4 synthesizes VLC saturated fatty acids (VLC-SFA) that are incorporated into several sphingolipids that provide the epidermal water barrier in the skin [7, 8, 9, 10] and into complex wax esters that contribute to the tear film generated by the Meibomian gland [11]. We found that the VLC-SFA, 28:0 and 30:0, are the predominant products of ELOVL4 in the brain as components of sphingolipids [12]. ELOVL4 also synthesizes VLC polyunsaturated fatty acids (VLC-PUFA) [4] as components of phosphatidylcholine (PC) that are enriched in retinal photoreceptor outer segments [13] in the retina and as components of sphingolipids in testes [12, 14, 15, 16].

ELOVL4 and its VLC-FA products are critical to the function of the central nervous system. Several mutations in the human ELOVL4 gene that cause neurological and skin disorders have been identified [1, 2, 17, 18, 19, 20, 21, 22]. Heterozygous inheritance of ELOVL4 mutations causes STGD3, an aggressive juvenile macular degeneration, in the absence of any other central nervous system or skin phenotypes [1, 2, 3]. Heterozygous inheritance of other ELOVL4 mutations causes autosomal dominant type 34 spinocerebellar ataxia (SCA34) and/or erythrokeratodermia variabilis (EKV) [17, 19, 20]; these patients show no retinal phenotype. Homozygous inheritance of ELOVL4 mutations causes devastating neurological disorders characterized by seizures, intellectual disability, spastic quadriplegia, ichthyosis, and pre-mature death [18, 21]. Thus, ELOVL4 and its VLC-FA products play a critical, albeit unknown role in brain development and function.

ELOVL4 is poised to play a role in many parts of the developing and mature brain. ELOVL4 localizes to the endoplasmic reticulum [5, 23] and is primarily expressed by neurons in the brain, although some expression of ELOVL4 may be present in glial cells, particularly oligodendrocytes [24]. Neuronal expression of ELOVL4 is widespread but varies in a region and cell type-specific manner. High levels of ELOVL4 are found in neurons of the cerebral cortex and portions of the hippocampus [24], consistent with the seizure phenotypes associated with homozygous inheritance of mutant ELOVL4. In particular, neurons in the CA3 region of the hippocampus, a structure intimately involved with epileptogenesis in a number of seizure disorders, show high levels of ELOVL4 [24]. Similarly, ELOVL4 is prominently expressed in the granule cells and Purkinje cells of the cerebellum [24], which is affected by the autosomal dominant mutations in ELOVL4 that cause SCA34 [17, 19, 20]. Expression of ELOVL4 in the brain is regulated at the genomic level [25]; it begins at embryonic stages and peaks shortly after birth before declining by 30 days after birth to low, but steady-state expression into adulthood [25]. The spatial and temporal regulation of ELOVl4 expression in the brain and the association of ELOVL4 mutations with varying degrees of human neural disease indicate that ELOVL4 and its VLC-FA products are critical to neuronal health and function.

In an attempt to identify the complex roles for ELOVL4 and its VLC-FA products in health and disease, our group developed a novel animal model to study the effects of ELOVL4 and VLC-FA depletion on brain function. Homozygous expression of mutations in Elovl4 or global deletion of Elovl4 in mice leads to their death within hours of birth due to dehydration [6, 7, 8, 9, 10], which until now, has prevented investigation into the function of ELOVL4 or its VLC-FA products. To circumvent this neonatal lethality, we generated skin-rescued (S + ) mice that express two non-functional copies of Elovl4 containing the 5-bp deletion found in STGD3 patients (797-801_AACTT) [1, 3], but with transgenic expression of the wild-type Elovl4 minigene in the skin under control of both the human skin-specific KERATIN-14 and INVOLUCRIN promoters, to rescue the skin barrier defect. These mice (S + Elovl4 mut/mut ) survived, but starting at post-natal day 19 (P19), developed a severe, progressive seizure phenotype that resulted in death by P21. This is consistent with the phenotype described of children with homozygous inheritance of ELOVL4 mutations [21]. Thus, we have developed a novel animal model that recapitulates the human condition, which permits for the first time investigation of the functional role of ELOVL4 and its VLC-FA products in the brain. The studies presented herein show that the absence of functional ELOVL4 and its VLC-FA products from the brain cause synaptic dysregulation and provide evidence that VLC-SFA are able to regulate pre-synaptic vesicle fusion kinetics.

Materials and Methods

Transgene Construction and Generation of S+Elovl4mut/mut and Control Mice

Three different transgenic mice were bred to generate the skin-rescued S + Elovl4 mut/mut mice. These included mice with heterozygous knock-in of the mouse Elovl4 gene containing the 5-bp (STGD3) deletion (Elovl4 wt/mut ) and transgenic mice expressing the mouse wild-type (wt) Elovl4 minigene under the human involucrin promoter, both of which have been previously described [9, 26]. We generated the third transgenic mouse line by expressing the mouse wt Elovl4 minigene under control of the human keratin-14 promoter pGEM3Z vector (kindly provided by Elaine Fuchs, PhD, Rockefeller University, New York, NY). The human keratin-14 (K14) promoter drives gene expression in the basal layer of the epidermis, outer root sheath cells of hair follicles, and in stratified squamous epithelia cells of the skin [27, 28]. To generate transgenic mice expressing the wt Elovl4 under the K14 promoter, wt mouse Elovl4 was PCR amplified using high-quality PCR enzymes (Thermo Fisher Scientific, Carlsbad, California) and pCMV-Elovl4 templates as previously described [4]. The PCR product was digested with Bam HI, purified, and cloned into the Bam HI site of the pGEM3Z vector containing the human K14 promoter to generate pGEM3Z-mouse-Elovl4 transgenic construct. The final construct was sequenced to verify proper orientation and sequence integrity of Elovl4. The K14-mouse-Elovl4-K14 polyA transgene cassette was digested with Eco RI and Hind III and used for generation of transgenic mice at Duke Neurotransgenic Laboratory Core (Duke University, Durham, NC). We characterized the TgK14-Elovl4 (Tg K14 Elovl4) transgenic founders by PCR. Expression of wt ELOVL4 in the skin was confirmed by western blotting.

To generate the S + Elovl4 mut/mut mice, we first crossed Elovl4 wt/mut mice with Tg K14 Elovl4 wt/wt and Tg INV Elovl4 wt/wt mice to generate Tg K14 Elovl4 wt/mut and Tg INV Elolv4 wt/mut mice, respectively. The Tg K14 Elovl4 wt/mut and Tg INV Elolv4 wt/mut were crossed to generate the skin-rescued Tg K14-INV (S + ) Elovl4 mut/mut (S + Elovl4 mut/mut ) mice and litter mate controls used in this study. During all crosses, mice from different parents were used. To promote survival of the S + Elovl4 mut/mut mice, pregnant females from the Tg K14 Elovl4 wt/mut and Tg INV Elolv4 wt/mut lines were maintained in an Ohmeda Medical Giraffe Incubator (Laurel, MD) until they gave birth and during the nursing period. The incubator temperature was maintained at 24 °C and the humidity held at 80–90%. Studies were performed using S + Elovl4 mut/mut mice and Elovl4 mut/mut mice (for embryonic culture) of both sexes and WT littermate controls of both sexes.

Animals and Husbandry

All experimental mice were bred into a C57B6 background. Mice were maintained in a pathogen-free barrier facility on a 12 h light:12 h dark daily cycle. Light intensity at cage level was ~ 150 lx. Food and water were available at all times. All animal procedures were approved by the University of Oklahoma Health Sciences Center Institutional Animal Care and Use Committee. All procedures conformed to the National Institute of Health Guide for the Care and Use of Laboratory Animals, the Association for Research in Vision and Ophthalmology Resolution on the Use of Animals in Research, and US Public Health Service guidelines.


Brains from S + Elovl4 wt/wt , S + Elovl4 wt/mut , and S + Elovl4 mut/mut mice were collected for histology and immunolabeling at post-natal days 19–21 (P19-P21, the period of seizure activity). At least five animals of each genotype were examined. Animals were euthanized by cervical dislocation followed by decapitation. The brains were removed from the skull and hemisected on an aluminum block half-submerged in liquid nitrogen. The left hemisphere of each brain was collected for biochemical analyses. The right hemisphere was embedded unfixed in optimal cutting temperature medium (OCT; Sakura Tissue Tek; VWR, West Chester, PA), frozen on the aluminum plate, and then stored at − 80 °C. Frozen sections (10 μm thickness) were prepared and collected onto Superfrost Plus slides (Fisher Scientific, Pittsburgh, PA) and stored at − 20 to − 30 °C until used.

For immunolabeling of brain tissue, cryosections were thawed and immersed in 100% methanol at − 30 °C for 20 min, rinsed in distilled water, and then rinsed in Hank’s buffered salt solution (HBSS). In some experiments, cryosections were subjected to high-temperature antigen retrieval in 10 mM citrate buffer (pH 6.0) for 30–60 min prior to rinsing in HBSS. Non-specific labeling was blocked for 2 h at room temperature using “blocker” solution (2–10% normal goat serum + 5% bovine serum albumin + 1% fish gelatin + 0.1–0.5% Triton X-100 in HBSS). Blocker was removed and a combination of primary antibodies raised in different host species was applied overnight at room temperature. Sections were rinsed in HBSS and incubated in an appropriate combination of fluorescently conjugated secondary antibodies for 60–75 min at room temperature. Sections were rinsed again and cover-slipped using Prolong Gold + DAPI (Life Technologies-Molecular Probes) to retard photobleaching.

For immunolabeling of cultured hippocampal neurons, cultured neurons grown on glass coverslips were fixed in 4% paraformaldehyde for 15–30 min at 4 °C, rinsed in HBSS, and then incubated in blocker for 45–60 min at room temperature to block non-specific labeling. Primary antibodies were applied for 4 h at room temperature or overnight at 4 °C, coverslips were rinsed, and appropriate fluorescent secondary antibodies were applied for 75 min at room temperature. Coverslips were rinsed and mounted onto glass slides using Prolong Gold with DAPI (Molecular Probes) and viewed by epifluorescence microscopy.

Specificity of labeling methods was confirmed by omitting primary antibody or substituting normal rabbit serum for primary antibody. Specimens labeled using only one primary antibody and a combination of secondary antibodies showed no bleed-through of signals between fluorescence channels.

For histological staining, frozen sections were thawed, rehydrated in HBSS, and then stained. Nissl staining was performed by applying a 1% toluidine blue solution to frozen sections of brain for 5–10 min on a hot plate at 60 °C. Sections were rinsed several times in HBSS at room temperature, cover-slipped using Prolong Gold, and observed on the microscope. Sudan Black B was prepared as a 0.3% solution in 70% ethanol, protected from light, and stored at 4 °C until used [29, 30]. A droplet of filtered Sudan Black B solution was applied to the sections on the slides, which were allowed to stand in a humidified chamber for 10 min at room temperature in the dark. Sections were then rinsed several times in HBSS at room temperature and cover-slipped using Prolong Gold and observed on the microscope.

Wide-field fluorescence and bright-field imaging were performed using an Olympus IX70 (Olympus America, Center Valley, PA) microscope fitted with a QiCAM CCD camera controlled via the QCapture software (QImaging, Surrey, BC) or, for low-magnification imaging, an Olympus MVX10 microscope fitted with an Olympus DP71 camera controlled via the CellSens software (Olympus America). Labeling patterns in fluorescence images were assessed by superimposing images of matching fields captured independently in each fluorescence channel. Low-magnification image montages were assembled using the CellSens or Photoshop software (Adobe Systems, San Jose, CA). To prepare figures, image scales were calibrated and images were imported into the Photoshop software. If necessary, brightness and contrast were adjusted uniformly across the image to highlight specific labeling.

Primary Antibodies for Immunolabeling

Affinity-purified rabbit polyclonal anti-ELOVL4 was raised against a synthetic peptide (aa 301-312) of wild-type mouse ELOVL4 conjugated to keyhole limpet hemocyanin [4]. This antibody recognizes the WT ELOVL4 but does not recognize the mutant form of ELOVL4 associated with STDG3 [4]. Specificity of this antibody has been confirmed by western blotting and pre-adsorption previously [4]. Deletion of WT Elovl4 eliminates immunolabeling [31, 32]. Anti-ELOVL4 was used at a dilution of 1:300 to 1:500.

Neuron-Specific Nuclear Protein (NeuN)

Mouse monoclonal anti-NeuN (Millipore, Cat# MAB377B; clone A60) recognizes three bands at 46–48 kDa corresponding to NeuN on western blots [33, 34] and labels most post-mitotic neurons immunohistochemically. Anti-NeuN was used at a dilution of 1:500.

Glutamic Acid Decarboxylase, 65 kDa Isoform (GAD-65)

Mouse monoclonal anti-GAD-65 (Millipore, Cat# MAB351; clone GAD-6) was raised against GAD purified from rat brain and recognizes a single band on western blots [35]. Anti-GAD-65 was used at a dilution of 1:300–1:500.

Active Zone

Pre-synaptic active zones were identified using a rabbit polyclonal antibody raised against recombinant Rim2 (aa 1-466) and affinity purified with a peptide corresponding to aa 41-59 of mouse Piccolo that recognizes a shared epitope in Rim1, Rim2, and Piccolo (Synaptic Systems, Gottingen, Germany, Cat# 364-003).

Vesicular Glutamate Transporter 1 (VGluT1)

Glutamatergic pre-synaptic terminals were immunolabeled using mouse monoclonal anti-VGluT1 that was raised against a fusion protein of aa 493-560 of rat VGluT1 diluted 1:100–1:200 (NeuroMab, Davis, CA. 75-066; clone N28/9).

Synaptic Vesicle Protein 2 (SV2)

Mouse monoclonal anti-SV2 was raised against purified synaptic vesicles and used at a dilution of 1:20–1:100 (Developmental Studies Hybridoma Bank, Cat# SV2, clone SV2. [36]).

Positron Emission Tomography (PET)

PET imaging for the measurement of 18F–labeled fluorodeoxyglucose (FDG) was performed by the Research Imaging Facility at the OUHSC College of Pharmacy. 18F-FDG was synthesized in a Biomarker Generator BG75 (Advanced Biomarker Technologies, Knoxville, TN, USA). Briefly, ~ 10 μCi/g 18F-FDG was delivered with a tail vein injection to anesthetized (2% isoflurane–air mixture) mice. Two hours after injection, the mice were re-anesthetized for imaging and positioned supine in a gantry of a PET-CT dual modality machine from Gamma Medica Ideas (Northridge, CA, USA). A fly-mode CT of brain was acquired before a 10-min long list-mode PET acquisition. Through the imaging period, the mice were kept anesthetized by a 2% isoflurane–air mixture. At 2.5 h post injection, blood was collected prior to euthanasia and collection of tissues. Radioactivity of the blood, heart, lung, spleen, liver, retina, and brain was measured, along with a fraction of the prepared dose for calculation of injected dose.

The acquired images were reconstructed by filtered back projection algorithm and fused with CT image to generate a composite PET-CT image using the AMIRA 3.1 software (FEI Visualization Sciences Group, Burlington, MA, USA). Composite images were used for segmentation-based drawing of a 3D region of interest surrounding the brain. No attempt was made to correct the images for attenuation.

The radioactive counts in the region of interest were determined as Ct (counts per unit volume). Ct decay was corrected to the time of injection and expressed as % injected dose per gram or per organ.


Mice were anesthetized with isoflurane and brains were harvested directly into liquid nitrogen by removal of the skull cap and rapid separation of the brain from the spinal cord using a pair of curved forceps (store at − 80 °C). In a cold room (4 °C), frozen brains were crush homogenized into powder while submerged in liquid nitrogen and stored at − 80 °C.

Separation and Quantification of ATP, ADP, AMP, NADH, and NADPH

Homogenized brain powder was extracted in 150 mM KOH and proteins were precipitated following incubation on ice (20 min) and then pelleted by centrifugation (10 min at 16,000×g). Supernatant was then filtered (0.45 μm pore size) prior to analysis. Analysis: Mobile phase solvent A [100 mM KH2PO4, 1.0 mM tetrabutylammonium sulfate (TBAS, pH 6.0)]; solvent B (acetonitrile (CH3CN). The injection was 100 μL and the flow rate was 1.0 mL/min. Column: Eclipse Plus C18 column with 5 μm diameter beads, 4.6 × 150 mm in length (Agilent). Elution conditions: stepwise gradients of buffer A/B [(1) 100%/0%, 0 to 2.5 min; (2) 95%/5%, 2.51 to 7.5 min; (3) 85%/15%, 7.51 to 15 min; and (4) 100%/0%, 15.1 to 25 min]. Detection: ATP, ADP, and AMP absorption at 254 nm. NADH and NADPH fluorescence excitation at 340 nm and emission at 430 nm.

Separation and Quantification of NAD+ and NADP+

Homogenized brain powder was extracted in 5% metaphosphoric acid (HPO3); proteins were precipitated following incubation on ice (20 min) and then pelleted by centrifugation (10 min at 16,000×g). Supernatant was then filtered (0.45 μm pore size) prior to analysis. Analysis: Mobile phase solvent A [100 mM KH2PO4, 1.0 mM TBAS, (pH 6.0)]; solvent B (Acetonitrile (CH3CN)]. The injection was 100 μL and the flow rate was 1.0 mL/min. Column: Eclipse Plus C18 column with 5 μm diameter beads, 4.6 × 150 mm in length (Agilent). Elution conditions: Stepwise gradients of buffer A/B [(1) 100%/0%, 0 to 5 min; (2) 85%/15%, 5.01 to 10 min; and (3) 100%/0%, 10.01 to 20 min].

Magnetic Resonance Imaging (MRI)

MRI experiments were performed using a Bruker Biospec 7.0 Tesla/30 cm horizontal–bore magnet imaging system (Bruker Biospin, Ettlingen, Germany). Animals were restrained by using 1.5–2.5% isoflurane at 0.8 L/min O2, placed in a 72-mm quadrature volume coil for signal transmission, and a surface coil was used for signal reception. For blood-brain-barrier permeability assessment, T1-weighted MR images (FLASH, TR = 60 ms, TE = 5.39 ms, 70° flip angle, 256 × 256 matrix, 4 steps per acquisition, 3.5 × 3.5 cm2 field of view, 1 mm slice thickness; spatial resolution of 137 μm × 137 μm) were obtained pre- and post-administration of Gd-DTPA (i.v. injection via the tail vein; 0.5 mol/L, 0.5 mL/kg body weight; Magnevist, Bayer HealthCare Pharmaceuticals, Wayne, NJ) at 2–5-min intervals over a 30-min time-course. Data processing: For determining BBB permeability, MR signal intensities were measured from regions-of-interest (ROIs) in brain tissue regions using the Paravision (Bruker) software.

Preparation of Synaptic Membranes from Baboon Brains

We used a modified version of the protocol described by VanGuilder et al. [37, 38]; see [39] for details. Briefly, five major membrane fractions were isolated along with a starting homogenate (H) from freshly dissected baboon hippocampus: P1 (nuclear), P2 (cytoskeletal), P3 (neurosynaptosomal), PSD (post-synaptic density), and SV (synaptic vesicle). Synaptic fractions were then re-suspended in Tris-HCl buffer (pH 7.4) and separated for electron microscopy, immunoblotting, or lipid analysis.

Electron Microscopy

Samples were fixed in a mixture of 2% paraformaldehyde and 2% glutaraldehyde in 0.1 M cacodylate buffer (pH 7.3) for 2 h on ice. The fixative was carefully rinsed out with three 0.1 M cacodylate buffer washes, keeping the pellet intact. The pellet was post-fixed in 1% osmium tetroxide in 0.1 M cacodylate buffer for 90 min at room temperature, rinsed, and dehydrated through an ethanol gradient and finally propylene oxide. Pellets were infiltrated with epon-araldite resin and heat-cured. Blocks were sectioned at 100 nm and sections were mounted on 300 copper mesh grids, stained with Sato’s lead to enhance contrast, and imaged on a Hitachi H-7600 transmission electron microscope.


Western blots were performed on 12% SDS-PAGE gels using standard electrophoresis methods. Immunoblotting for ELOVL4 in wild-type, heterozygous, and mutant animals was performed on hemisected brain homogenates (10 μg protein). ELOVL4 primary antibody (1:1000) was detected using a HRP anti-host secondary antibody (1:1000). β-Actin primary antibody (1:1000) was used with an HRP anti-host secondary antibody (1:3000) to re-probe for densitometry quantification of ELOVL4 levels. Homogenized synaptic fractions isolated from baboon hippocampus were loaded (10 μg protein). Confirmation of synaptic vesicle fraction identification was performed using primary antibodies (1:4000) against VGluT1 (rabbit clone #Bc66f), VGluT2 (rabbit clone #Dcf68), and NTT4 (rabbit anti-NTT4), all of which were kindly provided by Drs. Nicolas Bazan and Jeffery Erickson (LSU, New Orleans, LA). HRP anti-host secondary antibodies were used at a concentration of 1:2000. Blots were visualized using a Kodak Imager (Kodak Inc., Rochester, NY). The Carestream imaging software (Carestream Health, Inc., Rochester, NY, USA) was used to measure protein levels. Densitometry data were analyzed using GraphPad Prism 7 (GraphPad, La Jolla, CA).

Lipid Analysis

Total lipids from synaptic membrane fractions were extracted following the method of Bligh and Dyer [40] with modifications [41]. Fatty acid methyl esters (FAMES) were prepared, identified, and quantified as previously described [4]. Briefly, FAMES were prepared from total lipid extracts by subjecting them to strong acid hydrolysis (16.6% HCl in methanol at 85 °C overnight). Total FAMES were quantified using an Agilent Technologies 6890N gas chromatograph (GC) with a flame ionization detector (FID), using 15:0 and 17:0 as internal standards. VLC-SFA were quantified using an Agilent Technologies 7890 GC [41] with a 5975C inert XL mass spectrometer (MS) detector (Agilent Technologies). The GC-MS was operated in the electron impact (EI) single ion monitoring (SIM) mode. The 28:0 and 30:0 response values were obtained by using the m/z ratios 438.4 and 466.5, respectively, along with m/z 74.1 and 87.1. Sample concentrations were determined by comparison to external standards, using 25:0 and 27:0 as internal standards. Multivariate ANOVA with Tukey’s post hoc was used to determine statistical significance.

Extracellular Electrophysiology

Mice were euthanized and their brains carefully removed and placed for approximately 1 min in ice-cold oxygenated artificial cerebrospinal fluid (ACSF) solution containing 126 mM NaCl, 2.5 mM KCl, 1.25 mM NaH2PO4, 2 mM MgCl2, 2 mM CaCl2, 26 mM NaHCO3, 10 mM glucose, 2 mM pyruvic acid, and 0.4 mM ascorbic acid (final pH 7.4). After trimming away and applying a cut to the base (20 –30° angle), the brain was fixed to an ice-cold stage and placed in a HM650V vibrating microtome (Thermo Scientific, Burlington, ON, USA) filled with cold oxygenated slicing solution containing 240 mM sucrose, 25 mM NaCl, 2.5 mM KCl, 1.25 mM NaH2PO4, 26 mM NaHCO3, 0.4 mM ascorbic acid, 10 mM glucose, 10 mM MgCl2, and 2 mM pyruvic acid (final pH 7.4). The brain was sliced horizontally and hippocampal slices with a thickness of 350 μm were collected and transferred to a recovery chamber containing oxygenated ACSF. The slices were left in this chamber at 32 °C for 30 min and then at room temperature for at least 30 min. To record, the slices were positioned on a P5002A multi-electrode array (Alpha MED Scientific Inc., Osaka, Japan). The chamber was perfused with oxygenated ACSF at a rate of 2 mL/min at 32 °C. Six hundred (600) traces of network activity were recorded, each for a 1-s duration, under physiological conditions with continuous ACSF perfusion. For high K+ challenge to evoke epileptiform activity, the K+ concentration was increased to 7.5 mM in the ACSF. Field excitatory post-synaptic potentials (fEPSPs) were generated in the dentate gyrus (DG) region of the hippocampus by stimulating downstream electrodes along the perforant pathway. Input/output curves (I/O curves) were generated by applying increasing stimulus currents from 0 to 100 μA to the pathway and recording fEPSP responses. Calculation of I/O ratio was performed by dividing amplitude of evoked fEPSP by the amplitude of fiber valley and the resulting number was log normalized for statistical comparison. See below for details of extraction, quantification, and statistical analyses.

Data Processing

Standard testing methods, such as ANOVA with appropriate post hoc correction, Student’s t test, or Mann–Whitney exact test were employed when no data collection design embedding was involved.

For electrophysiology data, raw MED64 Mobius workflow files were opened and spikes were extracted in Mobius (© WitWerx Inc.). Positive and negative spike-threshold was set to + 0.021 and − 0.021 mV, respectively. Spike traces were extracted along with 1 ms of baseline before and after the spike event, without down sampling. Raw data were filtered using a Bessel highpass (2-pole) with a cutoff frequency of 1000 Hz and a DC filter with a typical spike length set to 1 ms. The resulting file containing all extracted spikes within that slice recording was then processed in Microsoft Excel using a visual basic macro that was coded and validated by us to extract each of the final parameters for statistical comparison.

The impact of genotype and K+ depolarization on the five variables of interest [amplitude (+), amplitude (−), inter-spike interval, frequency, and active frequency] was analyzed by fitting linear mixed effect models as implemented by the “lme” function in the R package “nlme.” The mixed-effects model extends the classical linear model (ANOVA/regression) to accommodate complex data collection design features such as nested layers and within-group correlation. The method formulation [42], computational method, and implementation of the model in R have previously been described [43]. The complex multilayer nested repeated data collection, with multiple channels/regions per slices and multiple slices per individual brains, was accounted for by proper specification of the random effect structure. Magnitude coefficient tables and p values for the significance of fixed effects were extracted using the tTable method, while confidence intervals were returned by the intervals function in the nlme package. In the figures, the 95% confidence intervals (CIs) for main effects and differences per region and total are represented as vertical lines, while the p values above the bars show the significance of interactions, which are the difference of these effects across mouse types or K+ treatment. When suitable, the dependent variables were pre-processed with boxcox transformation [44] to better fulfill the normality assumptions of the main statistical procedures.

Temporal variation of frequency over the 600-s observational period (see Fig. 8) was modeled and contrasted in the framework of generalized additive models [45], as implemented in the gam function of the R package mgcv. The function relies on smoothing splines for fitting the temporal curves and is able to deal with the random effects, capturing the complex data collection design as well. Spike occurrences were modeled as Poisson random events. The curve inserts in Fig. 5 depict the log of average process rates, the link functions of the Poisson family parameter, while the error bars show 95% CIs. Main effect curves (red, black) were derived with the plot_smooth function, while the differential effect (blue) was studied with the plot_diff function. The time intervals where the difference was significant, retrieved by the plot_diff function, are marked with horizontal bars at the bottom of the figure.

Primary Embryonic Hippocampal Cultures and Supplementation

Pregnant females were euthanized by cervical dislocation and embryonic day 18.5 (E18.5) embryos were removed into Hank’s solution + 20% NuSerum (Corning). Brains were removed and both hippocampi were micro-dissected under sterile conditions in a tissue culture hood and placed in fresh ice-cold Hank’s solution + 20% NuSerum. Both hemispheres were sliced into smaller subsections and transferred to 15 mL Falcon tubes. Each sample was washed three times with ice-cold Hank’s solution + 20% NuSerum and then three times with ice-cold Hank’s solution (allowing tissue to settle to the bottom between each wash). Hippocampal cells were then digested with 1 mL of pre-warmed digestion solution [140 mM NaCl, 5 mM KCl, 7 mM Na2HPO4, 2.5 mM HEPES + trypsin, and DNAse added fresh prior to use (final pH 7.4)] at 37 °C for 10 min before mechanical dissociation with flame-tapered/silicone-coated Pasteur pipettes. Trypsin was neutralized with an equal volume ice-cold Hank’s solution + 20% NuSerum and tissue was washed three times with ice-cold Hank’s solution + 20% NuSerum and then three times with ice-cold Hank’s solution (allowing tissue to settle to the bottom between each wash). Hippocampal cells were then dissociated with flame-tapered/silicone-coated Pasteur pipettes in 1 mL ice-cold dissociation solution (12 mM MgSO4·7 H2O in Hank’s solution + DNAse added fresh prior to use). Cells were then spun down for 5 min at 1200 rpm before being re-suspended in pre-warmed plating media and counted (Biorad, Hercules, CA automated cell counter). On day in vitro 0 (DIV0), 50,000 cells were plated per coverslip in 1 mL of plating media per well. On DIV1, a 500-μL 50% media change was done, replacing with 500 μL plating media. On DIV4, a 500-μL 50% media change was performed, replacing with 500 μL plating media + 4 μM of the mitotic inhibitor cytosine-arabinoside (ARA-C). Cells were subjected to FM1-43 imaging between DIV14-17. Supplementation: To assess the effects of re-supplying VLC-SFA, 24:0 or 28:0 + 30:0 SFAs were made into sodium salts, complexed to fraction V bovine serum albumin (BSA), and delivered to neurons in freshly prepared growth media + ARA-C at a concentration of 5 μg per milliliter. Supplementation (2.5 μg of each FA) was performed as a part of the standard DIV4 half media change (described above); after 1 week of co-incubation, another half media change was performed to reduce the amount of lipid in solution, and imaging was performed between DIV14-17 as before.

FM1-43 Dye Studies

We tested synaptic vesicle trafficking using amphipathic fluorescent styryl dyes of FM1-43 (Invitrogen, Carlsbad, CA). FM1-43 shows a robust increase of its quantum yield when incorporated into vesicles [46, 47]. This process is reversible, resulting in less free extracellular fluorescent dye in the perfusion solution. FM1-43 (4 μM) was loaded into the synaptic vesicles by depolarization for 90 s with 47 mM KCl containing Tyrode solution. After 10 min of wash with zero-Ca2+ Tyrode solution, neurons were stimulated with four rounds of 90 mM KCl containing Tyrode solution. Images were collected using an Olympus IX73 microscope, an Olympus 40× objective lens, and an Evolve-512 CCD camera, and analyzed by the MetaFluor imaging software (Molecular Devices, PA) as previously described [48, 49, 50, 51]. Fluorescence intensity was corrected for background fluorescence as detected after the experiment in each selected region. To compare release kinetics, starting fluorescence values were normalized for each synaptic bouton with the pre-stimulus level set to 1.


Depletion of VLC-SFA in the Brain Leads to Seizures and Pre-mature Lethality in Mice

Mice with global deletion (Elovl4 −/− ) or homozygous for STGD3 mutant Elovl4 (Elovl4 mut/mut ; 5-bp deletion: 797-801_AACTT) die shortly after birth from dehydration due to the loss of omega-O-acyl-ceramides that contain VLC-SFA, which are essential for epidermal water barrier function [7, 8, 9, 10]. The S + Elovl4 mut/mut mice we generated were rescued from neonatal lethality, but displayed a phenotype similar in many respects to that reported in human children with inherited homozygous ELOVL4 mutations [21]. At P19, S + Elovl4 mut/mut mice developed epileptic seizures that increased in frequency until their subsequent death at P21 (Online Resource 1). Compared to their WT littermate controls, S + Elovl4 mut/mut mice were developmentally delayed, with un-opened eyes and half the body weight of their heterozygous and WT littermates at P20 (Online Resource 2a), indicating an important role for ELOVL4 and its products during development. Interestingly, the wet weights of brains harvested from S + Elovl4 mut/mut mice at P20 did not differ significantly from their WT littermates (Online Resource 2b).

To determine the role of ELOVL4 in brain function, we characterized brain ELOVL4 expression by immunolabeling using a WT ELOVL4-specific antibody (Online Resource 3) that does not recognize the 5-bp del. mutant form of ELOVL4 [4]. The ELOVL4 staining pattern in brain sections from P19-P21, the period of seizure activity in S + Elovl4 mut/mut mice, revealed broad but region-specific neuronal expression of ELOVL4 in the brains of Elovl4 wt/wt and Elovl4 wt/mut mice (Fig. 1a), as we have previously reported [24]. In contrast, S + Elovl4 mut/mut mice showed no ELOVL4 labeling (Fig. 1a); residual labeling in the granule cell layer was not due to ELOVL4 as confirmed by western blotting (not shown). In Elovl4 wt/wt mice, ELOVL4 expression in the hippocampal formation was very strong in neurons in CA3, subiculum, and the hilus of the dentate gyrus (DG), while neurons in CA1 and CA2 showed substantially weaker ELOVL4 labeling (Fig. 1c), as reported previously [24]. The hippocampus in S + Elovl4 wt/wt , S + Elovl4 wt/mut , and S + Elovl4 mut/mut mouse brains showed normal light microscopic organization with no significant differences in size or morphology (Fig. 1c and Online Resource 4). We further confirmed loss of ELOVL4 expression in brain tissues of S + Elovl4 mut/mut mice by quantitative immunoblotting (Fig. 1b).
Fig. 1

Expression of ELOVL4 in the mouse brain a ELOVL4 expression in S + Elovl4 wt/wt , S + Elovl4 wt/mut , and S + Elovl4 mut/mut mice. b Western immunoblot probing for ELOVL4 in hemisected whole brain from S + Elovl4 wt/wt , S + Elovl4 wt/mut , and S + Elovl4 mut/mut mice normalized to β-actin and quantified by densitometry. Statistics: one-way ANOVA with Tukey’s multiple comparisons test, ****p < 0.0001 (n = 6) error ± SD. c Distribution of ELOVL4 (red) co-localized with the neuronal nuclear marker NeuN (green) in the hippocampal formation in S + Elovl4 wt/wt and S + Elovl4 mut/mut mice at P20. Cornu Ammonis field 3 (CA3), polymorph layer (arrow), Cornu Ammonis field 1 (CA1), dentate gyrus (DG), subiculum (Sub), fo (fornix), VL (lateral ventricle). Scale bar = 250 μm

Our preliminary studies indicated that synaptic function in the Schaffer collaterals and perforant path was dysregulated in S + Elovl4 mut/mut mice. Consistent with this finding, ELOVL4 expression is high in the CA3 region of the hippocampus and the entorhinal cortex, which give rise to the Schaffer collaterals and perforant path, respectively. The hippocampus has well-established links to many different types of seizure disorders, including medial temporal lobe epilepsy [52, 53]. This is due to the hippocampus serving as a major point of connection to cortex-associated regions that allows and facilitates the spread of epileptiform activity between cortical and hippocampal networks. Finally, the hippocampus is a tractable and well-defined experimental system in which to explore neurotransmission as it relates to epileptogenesis. For these reasons, we focused our studies on synaptic structure and function in the hippocampus of the S + Elovl4 mut/mut mice.

S+Elovl4mut/mut Mice Demonstrate Increased Energy Demand in the Brain

In view of the seizure and hyperactivity phenotype in S + Elovl4 mut/mut mice, we performed PET imaging on P19-21 mice to evaluate uptake of 18F-FDG, an indicator of cellular glucose demand in the brain. The PET results revealed a nearly threefold increase in the amount of glucose taken up into the brains of S + Elovl4 mut/mut mice compared to WT littermate controls, indicating increased metabolic demand in the brains of these seizure-prone S + Elovl4 mut/mut mice (Fig. 2a). Quantification of 18F accumulation in the brain and other control tissues harvested post-mortem, confirmed this finding (Fig. 2b).
Fig. 2

S + ELOVL4 mut/mut mice demonstrate increased energy demand and ATP production. a Qualitative positron emission tomography (PET) imaging of S + ELOVL4 wt/wt and S + ELOVL4 mut/mut mice. b Post-mortem tissue quantification of FDG radioactivity in S + ELOVL4 wt/wt and S + ELOVL4 mut/mut mice. Statistics: multiple t tests per row, Holm-Sidak’s multiple comparisons correction, ****p < 0.0001. c HPLC assessment and quantification of general intermediary metabolites and energy charge (E.C.) in whole brain from S + ELOVL4 wt/wt and S + ELOVL4 mut/mut mice. Statistics: multiple t tests per row, Holm-Sidak’s multiple comparisons correction, **p < 0.01. d Magnetic resonance imaging with the gadolinium-based contrast agent revealed no abnormal uptake in the brains of S + ELOVL4 mut/mut mice compared to wild-type controls

Increased FDG uptake can be indicative of elevated energy demand or disruption of the blood-brain barrier (BBB). We assessed both possibilities by analyzing ATP levels by HPLC and structural integrity of the BBB using magnetic resonance imaging (MRI) with Gd-DTPA, respectively. Brains of S + Elovl4 mut/mut mice showed a threefold increase in ATP with no significant change in the other intermediary metabolites compared to WT littermate controls (Fig. 2c). To assess the integrity of the electron transport chain, we evaluated complex I activity using a fluorometric NADH oxidase assay. There were no differences between genotypes for complex I activity (not shown). MRI with Gd-DTPA contrast enhancement revealed no evidence for differences in BBB permeability in S + Elovl4 mut/mut mice compared to WT littermate controls (Fig. 2d). Collectively, these results suggest that the increase in ATP levels may simply reflect the large energy requirement associated with seizure activity.

VLC-SFA Are Enriched in Synaptic Vesicles

To determine the effect of Elovl4 depletion on brain lipids, we analyzed the glycerophospholipids (GPL) and sphingolipids (SPH) from hippocampus of P20 Elovl4 wt/wt and S + Elovl4 mut/mut mice using GC-MS and triple quadrupole tandem MS. The predominant VLC-FA in Elovl4 wt/wt mouse brain were 28:0 and 30:0 VLC-SFA. To determine the subcellular localization of VLC-SFA in the hippocampus, we prepared synaptic vesicles (SV) and other fractions from freshly dissected baboon hippocampus. Baboon brains were obtained post-mortem and chosen for these studies to ensure that enough material was obtained for lipidomics following fractionation. Membrane fractions were confirmed by transmission electron microscopy (Fig. 3a–d) and western blots (Online Resource 5). Lipidomic analysis revealed that both 28:0 and 30:0 were enriched in synaptic vesicle membranes compared to other membrane fractions (Fig. 3e). Low relative levels of VLC-SFA in the starting homogenate, neurosynaptosomal, and post-synaptic density fractions reflect the low abundance of VLC-SFA-containing species relative to the other lipid species present in these fractions.
Fig. 3

Brain-derived ELOVL4 products are 28:0 and 30:0 that are enriched in synaptic vesicle membranes. Electron micrographs of synaptic fractions isolated from baboon hippocampus by sucrose gradient centrifugation (scale bar = 500 nm). a Starting homogenate (Homo.) with a single neurosynaptosomal unit (arrow). b Neurosynaptosomal fraction (Synapt.) with multiple neurosynaptosomes in frame (arrows). c Post-synaptic density fraction (PSD) with multiple isolated densities indicated (arrows). d Synaptic vesicle fraction (SV) with high purity, vesicle indicated in zoomed inset (arrow). e Lipidomic analysis (GC-MS followed by GC-FID) reveals enrichment of both 28:0 and 30:0 in synaptic vesicle membranes relative to the other synaptic fractions. Statistics: two-way ANOVA with Tukey’s multiple comparison test, ****p < 0.0001 (n = 3) error ± SEM

VLC-SFA Deficiency Causes Dysregulated Pre-synaptic Vesicle Fusion

To assess the influence of VLC-SFA on synaptic vesicle fusion kinetics, we performed FM1-43 dye studies [47, 50, 54] to measure pre-synaptic vesicle fusion rates in primary hippocampal neuronal cultures from non-skin-rescued E18.5 embryos from Elovl4 wt/wt and Elovl4 mut/mut mice. Hippocampal neurons cultured from Elovl4 wt/wt and Elovl4 mut/mut embryos formed synapses, as indicated by the presence of synaptic vesicle clusters and active zones, which are only assembled in the presence of a post-synaptic terminal, demonstrating that WT ELOVL4 is not required for synapse formation (Fig. 4). Cultured neurons of both genotypes formed glutamatergic (Fig. 4g–l) and GABAergic synapses (Fig. 4m–r). Furthermore, there were no overt differences in synapse formation between genotypes. As expected, immunolabeling confirmed that ELOVL4 was expressed in neurons cultured from Elovl4 wt/wt mice, while neuronal cultures from Elovl4 mut/mut mice showed no labeling for WT ELOVL4 (Online Resource 6).
Fig. 4

Cultured hippocampal neurons develop synapses in the absence of WT ELOVL4 with formation of both excitatory glutamatergic and inhibitory GABAergic synapses Hippocampal neurons cultured from Elovl4 wt/wt and Elovl4 mut/mut embryos all formed pre-synaptic terminals in vitro (arrowheads) as shown by labeling for SV2 (a, b), a ubiquitous synapse marker; VGluT1 (c, d), a marker for glutamatergic terminals; and GAD-65 (e, f), a marker for GABAergic terminals. Double labeling for VGluT1 and the pre-synaptic active zone (AZ) confirmed glutamatergic synapse formation (arrowheads) by hippocampal neurons cultured from Elovl4 wt/wt and Elovl4 mut/mut embryos (gl). Double labeling for GAD-65 and the pre-synaptic active zone confirmed GABAergic synapse formation (arrowheads) by hippocampal neurons cultured from Elovl4 wt/wt and Elovl4 mut/mut embryos (mr). Scale bars = 20 μm for all panels

To test whether the enrichment of VLC-SFA in synaptic vesicle membranes affected pre-synaptic function, we performed a detailed assessment of synaptic vesicle fusion kinetics in individual synapses using FM1-43 dye [46, 47, 49, 50, 51, 54]. Loading and release of FM1-43 dye from synaptic vesicles was driven with depolarizing high K+ solution [50]. Analysis of synaptic vesicle fusion was performed between DIV14-17 on samples of over 2200 individual synapses per genotype (n = 9 cultures per genotype). Neurons from Elovl4 mut/mut hippocampus showed faster pre-synaptic release of FM1-43 dye than neurons from WT control hippocampus (Fig. 5a, c). Interestingly, this shift of cumulative release frequency was not achieved by a general acceleration of all pre-synaptic neurotransmission, but rather by what appears to be selective acceleration of synaptic vesicle fusion in a subset of synapses in the absence of VLC-SFA. The fact that different synaptic populations respond to the Elovl4 mutation differently fits with the observation that not all hippocampal neurons express ELOVL4. In addition, assessment of total fluorescence change revealed that the recycling synaptic vesicle pool was smaller in Elovl4 mut/mut synapses than in WT synapses (Fig. 5d).
Fig. 5

Dysregulation of synaptic vesicle release in mutant neurons lacking ELOVL4. FM1-43 fluorometric assessment of synaptic vesicle release rates and pool size in E18.5 primary hippocampal cultures collected from Elovl4 wt/wt and Elovl4 mut/mut embryos +/− treatment with either 28:0 + 30:0 or 24:0. a Representative destaining curves comparing release rates in WT (black) and mutant animals (red) in response to high K+ depolarization. b Representative destaining curves comparing release rates in mutant animals supplemented with either 24:0 (blue) or 28:0 + 30:0 (green) in response to high K+ depolarization. c Cumulative distribution of release rates for all synapses measured (Kolmogorov–Smirnov non-parametric examination of equality, p < 0.001). Inset: Frequency distribution of responses with slowest responding synapses falling to the left and the fastest to the right on the curve. d Cumulative distribution of the recycling pool of synaptic vesicles measured as total fluorescence released during the course of the experiment for all synapses measured. Inset: Frequency distribution of total fluorescent load turned over by each synapse with the synapses made up of the smallest pool at any given moment in time falling to the left, and those synapses with a larger pool at any given moment falling to the right of the curve

To distinguish any pleiotropic effects of the genetic manipulation from VLC-SFA deficiency arising from the inactivity of the mutant Elovl4 on synaptic vesicle fusion kinetics, we supplemented neuronal cultures with an equimolar mixture of the two major ELOVL4 products in the brain (28:0 + 30:0), or with 24:0, a precursor for ELOVL4 elongation present in neurons of both genotypes, which served as a control long-chain (LC)-SFA. Assessment of Elovl4 mut/mut synaptic vesicle fusion kinetics in the presence of 28:0 + 30:0 VLC-SFA (1600+ individual synapses per genotype; n = 10 cultures) showed rescue of synaptic release kinetics, shifting the release rate curve back to wild-type levels (Fig. 5b, c). This demonstrates that VLC-SFA regulate pre-synaptic release kinetics. Conversely, supplementation with the LC-SFA 24:0 (900+ individual synapses; n = 10 cultures) did not affect the release kinetics of Elovl4 mut/mut synapses (Fig. 5c). Together, these results indicate that the absence of the VLC-SFA rather than the presence of the mutant STGD3 ELOVL4 protein is responsible for the pre-synaptic dysregulation observed in Elovl4 mut/mut neurons. Unexpectedly, supplementation with 24:0 or 28:0 + 30:0 SFA did not rescue cumulative FM1-43 fluorescence uptake, which reflects the size of the synaptic vesicle pool (Fig. 5d). This suggests that this particular observation may be a secondary developmental or regulatory factor arising from the fact that these neurons still developed from E7.5 (onset of Elovl4 expression) [25] until DIV4 without VLC-FA.

S + Elovl4 mut/mut Mice Show Aberrant Neuronal Firing Patterns Under Spontaneous and Evoked Conditions

To better understand the epileptiform activity in the brains of S + Elovl4 mut/mut mice, we performed spontaneous and evoked extracellular hippocampal field recordings. Using a 64 channel multi-electrode array, we assessed activity in the hippocampus as a whole as well as within specific sub-regions (DG, CA3, and CA1). Field potential recordings (600 consecutive 1 s traces) were performed in hippocampal slices and extracted spikes were analyzed for frequency, inter-spike interval, and amplitude to assess network activity (Fig. 6).
Fig. 6

Altered hippocampal network properties and spontaneous activity in Elovl4 mut/mut mice. Extracellular electrophysiology under physiological conditions in hippocampal slices ex vivo collected from S + Elovl4 wt/wt and S + Elovl4 mut/mut mice. The following measurements were made during 600 trace (1 s/trace) recordings of extracellular field potentials in hippocampal slices perfused with normal ACSF at 37 °C (see also suppl. Video 3). a Spontaneous frequency as a measure of spikes/s. b Spontaneous inter-spike interval (ISI) as a measure of time between spikes. c “Active” spontaneous frequency as a measure of spikes/s of activity. d Amplitude (+) spikes as a measure of spike magnitude (mV). e Amplitude (−) spikes as a measure of spike magnitude (mV). See methods for detailed statistics (WT: n = 7, slice # = 13; mut: n = 14, slice # = 34) error ± 95% confidence interval. f The input/output ratio in response to stepwise increased stimulation (20 μA minus 100 μA). Note logarithmic normalization on y-axis (statistics: two-way RM ANOVA, *p < 0.05 from 70 to 100 μA, error ± 95% confidence interval. WT: n = 3; mut: n = 10)

Under normal artificial cerebral spinal fluid (ACSF) conditions (2.5 mM K+), recording of spontaneous extracellular hippocampal field potentials confirmed a burst-like firing pattern in slices from S + Elovl4 mut/mut animals distinct from the more sporadic, tonic firing patterns observed in WT littermate controls. In two cases, slices from S + Elovl4 mut/mut mice displayed spontaneous epileptiform activity (Online Resources 7 and 8). However, S + Elovl4 mut/mut hippocampal slices showed decreased average frequency of spontaneous network events overall compared to WT control slices (Fig. 6a). This bursting activity could initiate spontaneous spreading epileptiform activity throughout the whole hippocampus under physiologic conditions. Indeed, the inter-spike interval in S + Elovl4 mut/mut slices was significantly reduced compared to WT controls, demonstrating a shift from a variable sporadic activity pattern in control slices to a predominately burst-like response in the mutant animals (Fig. 6b). To further analyze the pattern of responses in S + Elovl4 mut/mut mice, we calculated the spontaneous frequency of activity, for which we divided the number of spikes by the duration of their activity rather than the duration of the entire recording. This measurement revealed that despite the decrease in overall frequency, when neurons in S + Elovl4 mut/mut slices fire, they do so with a significantly higher frequency of activity (Fig. 6c), indicating that the hippocampus of mutant animals showed distinct periods of burst-like responses with a high frequency of activity, separated by periods of low activity or silence. The average spike amplitude under physiological conditions also was significantly lower in S + Elovl4 mut/mut slices compared to WT controls (Fig. 6d, e).

Given the observation of spontaneous epileptiform activity in mutant slices (Online Resource 8), we tested whether driving activity in mutant slices using a depolarizing stimulus evoked similarly enhanced neuronal activity compared to controls, by artificially elevating the probability of release. First, we compared the evoked synaptic responses following electrode stimulation in DG, which receives the main input from temporal cortex via the perforant path. We recorded excitatory post-synaptic field potentials (fEPSPs) evoked by electrode stimulation using a series of stepwise increased stimuli up to 100 μA. Synaptic I/O ratios showed significantly enhanced synaptic transmission in slices from S + Elovl4 mut/mut mice compared to WT littermate controls (Fig. 6f). Second, we induced global, synchronized depolarization using ACSF with high potassium (7.5 mM K+) (Figs. 7 and 8) and repeated the multi-electrode array recordings. Field recordings obtained under physiological ACSF conditions and under depolarizing high K+ conditions showed a dramatic difference in network activation between S + Elovl4 mut/mut slices and WT control slices. As expected, under depolarizing conditions, S + Elovl4 mut/mut slices showed strong activation, with higher evoked spike frequency than WT controls (Fig. 7a). The inter-spike interval (ISI) in S + Elovl4 mut/mut slices showed no difference between normal and high K+ conditions, suggesting that the mutant hippocampus was limited to burst-like responses regardless of the degree of depolarization. In contrast, WT control hippocampus showed reduced ISI in response to elevated K+, shifting to a more burst-like response, as expected (Fig. 7b). The average fEPSP amplitude for positive spikes under high K+ conditions increased in S + Elovl4 mut/mut slices compared to WT control slice. Thus, when pre-synaptic release is synchronized, S + Elovl4 mut/mut neurons generate a significantly larger positive fEPSP amplitude response than the WT controls and the magnitude of this difference was much larger downstream in CA3 and CA1 than it was in DG (Fig. 7c). Interestingly, the fEPSP amplitude response for negative spikes showed the opposite effect with a larger negative amplitude response in the WT control slices and in this case, the magnitude of this difference was much larger upstream in DG compared to CA3 and CA1 (Fig. 7d).
Fig. 7

Extracellular electrophysiology under physiological conditions followed by depolarizing conditions in hippocampal slices ex vivo collected from S + Elovl4 wt/wt and S + Elovl4 mut/mut mice. The following measurements were made during 600 trace (1 s/trace) recordings of extracellular field potentials in hippocampal slices perfused with physiological ACSF (normal ACSF = 2.5 mM K+) followed immediately by a second 600 trace (1 s/trace) recording during which perfusion was switched to depolarizing, higher extracellular potassium ACSF (high K+ ACSF = 7.5 mM K+) at time = 20 s. a Evoked frequency presented as the difference between spikes/s at high K+ ACSF and spikes/s at normal K+. b Evoked inter-spike interval (ISI) presented as the time difference between spikes at high K+ and spikes at normal K+. c Evoked amplitude (+) spikes presented as the difference between spike magnitudes (mV) in high K+ and normal K+. d Evoked amplitude (−) spikes presented as the difference between spike magnitudes (mV) at high K+ and normal K+. See methods for detailed statistics (WT: n = 9, slice # = 22; mut: n = 9, slice # = 22) error ± 95% confidence interval

Fig. 8

Uncontrolled spread of epileptiform activity under depolarizing condition to CA1 hippocampal region in Elovl4 mut/mut mice. a Frequency matrix (all 64 channels × 600 s) as total spikes/s/channel (high K+ ACSF perfusion begins at t = 20 s). Inset: Sum of all regions. Spline smoothed curves of log frequency with 95% confidence bands; intervals over which the difference is significant are marked by a blue bar below. b Frequency matrix (all DG channels × 600 s) as total spikes/s/DG channel (high K+ ACSF perfusion begins at t = 20 s). Inset: DG region. Spline smoothed curves of log frequency with 95% confidence bands; intervals over which the difference is significant are marked by a blue bar below. c Frequency matrix (all CA3 channels × 600 s) as total spikes/second/CA3 channel (high K+ ACSF perfusion begins at t = 20 s). Inset: CA3 region. Spline smoothed curves of log frequency with 95% confidence bands; intervals over which the difference is significant are marked by a blue bar below. d Frequency matrix (all CA1 channels × 600 s) as total spikes/s/CA1 channel (high K+ ACSF perfusion begins at t = 20 s). Inset: CA1 region. Spline smoothed curves of log frequency with 95% confidence bands; intervals over which the difference is significant are marked by a blue bar below. See methods for detailed statistics (WT: n = 9, slice # = 22; mut: n = 9, slice # = 22) error (insets) ± 95% confidence interval

Temporal analysis of the responses to high K+ stimulation revealed striking differences between S + Elovl4 mut/mut and WT hippocampus as a whole and among hippocampal sub-regions (Fig. 8). Onset of activity in DG (Fig. 8b) in response to high K+ was significantly faster in the S + Elovl4 mut/mut hippocampus compared to WT control hippocampus. Despite high activity levels in the DG of WT slices, there was no subsequent downstream increase in activity in CA3 or CA1 (Fig. 8c, d). This is in stark contrast to the increased downstream activity in CA3 and CA1 of the S + Elovl4 mut/mut hippocampus. These findings are consistent with the significantly higher negative spike amplitudes in DG for the WT control animals (Fig. 7d). Critically, this downregulation of activity seen in the WT control hippocampus animals was entirely absent from the S + Elovl4 mut/mut hippocampus. Of particular interest, the CA1 region in the S + Elovl4 mut/mut hippocampus maintained a level of high activity in response to K+ depolarization compared to the wt control hippocampus (Fig. 8d), consistent with the increased positive spike amplitude observed in the CA1 region of the S + Elovl4 mut/mut hippocampus under high K+ stimulation (Fig. 7c).


This report establishes a double transgenic mouse model, the S + Elovl4 mut/mut mouse, with homozygous knock-in of the Stargardt-like macular dystrophy (STGD3) mutation of Elovl4 and skin-specific rescue of WT Elovl4 expression to prevent neonatal lethality, that recapitulates critical aspects of the devastating central nervous system dysfunction associated with homozygous inheritance of ELOVL4 mutations in humans. Critically, S + Elovl4 mut/mut mice develop seizures similar to those seen in the human disease that appear by P19 and lead to death by P21. Electrophysiological analysis of hippocampal slices showed spontaneous epileptogenic activity in the S + Elovl4 mut/mut hippocampus and aberrant neurotransmission through the principle circuit of the hippocampus. Dye imaging studies showed accelerated pre-synaptic release kinetics in individual synaptic terminals of cultured S + Elovl4 mut/mut hippocampal neurons. Aberrant synaptic release in these cells was rescued to WT levels by supplementation of VLC-SFA via the culture medium, but not by LC-SFA. These studies establish a previously unrecognized role for ELOVL4 and its VLC-SFA products as regulators of pre-synaptic release kinetics and epileptogenesis.

A key attribute of the S + Elovl4 mut/mut mouse model is that it recapitulates the severe seizure phenotype of human syndromes that arise from homozygous inheritance of mutant ELOVL4. Our PET and metabolic studies also revealed that the S + Elovl4 mut/mut mouse brain has greatly elevated energy demands and elevated ATP levels compared to the brains of WT littermate control mice. The BBB remained intact in S + Elovl4 mut/mut mice, suggesting that the increased energy demands reflect the seizures and elevated neural activity observed in these animals. Under prolonged neuronal activation, the brain will utilize the astrocyte-neuron lactate shuttle to try and sustain their energy requirement via conversion of glucose to lactate to be used as an additional energy substrate for oxidative-derived ATP production [55]. The seizures and metabolic abnormalities that characterize the S + Elovl4 mut/mut brain occur in the absence of any gross defects in brain size, structure, or organization, suggesting that VLC-SFA deficiency had little effect on cell proliferation or migration in the developing brain.

In contrast, functional ELOVL4 and VLC-SFA are essential for normal synaptic function. Our studies of cultured hippocampal neurons indicate that functional ELOVL4 and its VLC-SFA products are not essential for formation of glutamatergic or GABAergic synapses. However, FM1-43 dye imaging experiments to visualize pre-synaptic release kinetics showed that synapses made by S + Elovl4 mut/mut neurons exhibited accelerated kinetics from a subpopulation of synapses. Critically, re-supply of 28:0 and 30:0 via the medium rescued this synaptic release kinetics back to WT control levels, indicating that the defect arose from VLC-SFA deficiency rather than the presence of mutant ELOVL4. Furthermore, the effect on pre-synaptic release was not rescued by supplying 24:0, a precursor for ELOVL4-mediated synthesis of VLC-SFA. Thus, functional ELOVL4 is essential for VLC-SFA synthesis, consistent with previous biochemical studies [4, 5, 23]. A critical unresolved question is the identity of the specific synapses that show aberrant pre-synaptic release kinetics in the absence of VLC-SFA. CA3 pyramidal cells show the highest ELOVL4 levels in the hippocampus, which makes their synapses onto the CA1 pyramidal cells via the Shaffer collaterals excellent candidates to have aberrant release kinetics and contribute to epileptogenesis.

The aberrant synaptic release kinetics observed in the FM-dye release experiments are consistent with the spontaneous seizure activity and aberrant network responses observed in S + Elovl4mut/mut hippocampal slices. The striking difference in neuronal activity seen in mutant slices during normal vs. high K+ ACSF conditions may reflect dysregulated summation [56, 57, 58, 59]. The observed pattern of spontaneous activity may represent an uncoupling of the neuron’s control over the timing and duration of its pre-synaptic release. Although the overall spike rate in the S + Elovl4mut/mut hippocampal slices under normal ACSF conditions is reduced compared to WT controls, neural activity in S + Elovl4mut/mut hippocampal slices in the absence of VLC-SFA shifts to a pronounced bursting activity pattern that is not observed in the WT slices. This bursting activity is a potential substrate for seizure formation, in that over time the synchronization of these bursting evens would produce highly coordinated bursts of neurotransmitter release in the S + ELOVL4 mut/mut hippocampus, enhancing synaptic summation and increasing the likelihood of reaching the threshold to initiate seizure activity. This is especially true in the CA1 region of the hippocampus, which receives the largest number of pre-synaptic inputs from the ELOVL4 positive neurons in the CA3.

Mutations in the Drosophila ceramidase gene, slab, cause a loss of readily releasable vesicles as shown by FM1-43 dye studies [60]. TEM of synapses isolated from these flies revealed an increase in linked synaptic vesicles tethered at the plasma membrane, but unable to fuse. Ceramidase enzymes cleave esterified fatty acids from molecules with a sphingosine backbone [61]. In brain tissue, this class of enzymes demonstrated a significantly higher cleavage preference for longer chain saturated fatty acids [61]. Regulation of the concentration of these saturated fatty acids within SV membranes by ongoing cleavage and esterification of different length acyl chains may fine-tune pre-synaptic release; the higher the concentration of VLC-SFA, the more rigid and less fusible SV membranes may be. Confirming this concept, but using PUFA, which would impose the opposite effect (increased membrane fusion), FM1-43 dye studies revealed that the longer and more polyunsaturated the fatty acid supplemented, the more FM1-43 dye accumulated in the vesicles within the cell, indicating faster vesicle fusion and turnover [62]. These studies support the notion that synaptic vesicle membrane fatty acid composition may be an important factor in the kinetics of neurotransmitter release.

The molecular mechanism by which VLC-SFA regulates the kinetics of pre-synaptic vesicle release is currently unknown. One possible explanation is that because of their length and the absence of any cis double bonds, VLC-SFA could extend through the lipid bilayer and interact with fatty acyl chains esterified to glycerophospholipids and sphingolipids in the opposing bilayer. Such acyl-acyl hydrophobic interactions across the lipid bilayer could increase the van der Waals forces within the bilayer, thereby stabilizing the membranes and resisting fusion with other membranes. The absence of these interactions, which would result from the loss of functional Elovl4 in the S + Elovl4 mut/mut mice, could increase the probability of release events such as we observed in the current study. However, follow-up studies aimed at identifying the mechanism by which the absence of VLC-SFA alters synaptic vesicle fusion kinetics will be of critical importance moving forward. Interestingly, our results suggest a role for VLC-SFA in synaptic release that is markedly different from that described for cholesterol, which facilitates synchronized evoked transmitter release [63, 64]. Such regulatory function of VLC-SFA in synaptic transmission is novel and markedly different from other lipid or lipophilic substances previously tested that acted via a receptor. For instance, platelet-activating factor (PAF) has been shown to serve a critical modulatory effect on pre-synaptic events, but all of its effects, including an influence on long-term potentiation and memory formation, were prevented by PAF receptor inhibitors [65, 66, 67, 68].

In summary, we have identified a previously unknown role for VLC-SFA as regulators of synaptic vesicle release. These studies demonstrate that the absence of 28:0 and 30:0 causes dysregulated pre-synaptic release kinetics in hippocampal neurons by some yet-to-be determined mechanism. This disruption in synaptic transmission is one possible mechanism underlying the severe epileptiform seizures that arise from VLC-SFA deficiency. These novel findings raise further questions that must be addressed.



The authors thank the following individuals for their various contributions to this work: Wojciech Kedzierski for providing the Elovl4 wt/mut and transgenic mice expressing the mouse WT ELOVL4 under the involucrin promoter; Nicolas Bazan for providing antibodies (VGluT1, VGluT2, and NTT4), as well as for the intellectual discussion; Mark Dittmar for animal care oversight as well as for specialized housing facilities construction and management; Willard Freeman, William Sonntag, Nawajes Mandal, Sreemathi Logan, and Nicole Ashpole for their intellectual discussions; Raju Rajala for the critical review of this manuscript and intellectual discussion; Faizah Bhatti for providing the initial neonatal incubator for housing experimental mice; Gary White, Roman Wolf, and Madeline Buddha for providing baboon brains; Ben Fowler at the OMRF Imaging Facility for the expertise and use of TEM equipment; Megan Stiles, Negar S. Rahman, Fauzziya Muhammad, Andria Hedrick, Nataliya Smith, Debra Saunders, Clair Crewe, and Albert Orock for the technical assistance; Joel McRae, Dallas Barnet, and Adeline Machalinski for managing the breeding and maintenance of all animal lines.

The monoclonal antibody against VGluT1 (clone N28/9) was developed by and/or obtained from the UC Davis/NIH NeuroMab Facility, supported by NIH grant U24NS050606 and maintained by the Department of Neurobiology, Physiology and Behavior, College of Biological Sciences, University of California, Davis, CA, 95616. The monoclonal anti-Synaptic Vesicle protein 2 (SV2) developed by K Buckley and RB Kelly was obtained from the Developmental Studies Hybridoma Bank, created by the NICHD of the NIH and maintained at The University of Iowa, Department of Biology, Iowa City, IA, 52242.


This work was supported by National Institutes of Health Grants R01EY00871, R01EY04149, R21NS090117, and P30EY021725 to REA; F31NS089358 to BRH; Reynolds Oklahoma Center on Aging Collaborative Grant to REA and Fellowship to BRH; Research to Prevent Blindness (Departmental); Presbyterian Health Foundation to FD; and Knights Templar Eye Foundation and Bright Focus Foundation Inc. grants to MPA.

Compliance with Ethical Standards

Conflict of Interest

Dr. Hopiavuori, Dr. Anderson, Dr. Agbaga, and Mr. Brush have a US Patent application (US20170014365) for the use of VLC-SFA in the treatment of human disease.

Supplementary material

12035_2017_824_MOESM1_ESM.mp4 (7.1 mb)
ESM 1 (MP4 7262 kb)
12035_2017_824_MOESM2_ESM.mp4 (3.4 mb)
ESM 2 (MP4 3451 kb)
12035_2017_824_MOESM3_ESM.mp4 (6.6 mb)
ESM 3 (MP4 6717 kb)
12035_2017_824_MOESM4_ESM.pdf (670 kb)
ESM 4 (PDF 669 kb)


  1. 1.
    Zhang K, Kniazeva M, Han M, Li W, Yu Z, Yang Z, Li Y, Metzker ML et al (2001) A 5-bp deletion in ELOVL4 is associated with two related forms of autosomal dominant macular dystrophy. Nat Genet 27(1):89–93. CrossRefPubMedGoogle Scholar
  2. 2.
    Bernstein PS, Tammur J, Singh N, Hutchinson A, Dixon M, Pappas CM, Zabriskie NA, Zhang K et al (2001) Diverse macular dystrophy phenotype caused by a novel complex mutation in the ELOVL4 gene. Invest Ophthalmol Vis Sci 42(13):3331–3336PubMedGoogle Scholar
  3. 3.
    Edwards AO, Donoso LA, Ritter R 3rd (2001) A novel gene for autosomal dominant Stargardt-like macular dystrophy with homology to the SUR4 protein family. Invest Ophthalmol Vis Sci 42(11):2652–2663PubMedGoogle Scholar
  4. 4.
    Agbaga MP, Brush RS, Mandal MN, Henry K, Elliott MH, Anderson RE (2008) Role of Stargardt-3 macular dystrophy protein (ELOVL4) in the biosynthesis of very long chain fatty acids. Proc Natl Acad Sci USA 105(35):12843–12848. CrossRefPubMedPubMedCentralGoogle Scholar
  5. 5.
    Logan S, Agbaga MP, Chan MD, Brush RS, Anderson RE (2014) Endoplasmic reticulum microenvironment and conserved histidines govern ELOVL4 fatty acid elongase activity. J Lipid Res 55(4):698–708. CrossRefPubMedPubMedCentralGoogle Scholar
  6. 6.
    Uchida Y, Holleran WM (2008) Omega-O-acylceramide, a lipid essential for mammalian survival. J Dermatol Sci 51(2):77–87.
  7. 7.
    Cameron DJ, Tong Z, Yang Z, Kaminoh J, Kamiyah S, Chen H, Zeng J, Chen Y et al (2007) Essential role of Elovl4 in very long chain fatty acid synthesis, skin permeability barrier function, and neonatal survival. Int J Biol Sci 3(2):111–119CrossRefPubMedPubMedCentralGoogle Scholar
  8. 8.
    Li W, Sandhoff R, Kono M, Zerfas P, Hoffmann V, Ding BC, Proia RL, Deng CX (2007) Depletion of ceramides with very long chain fatty acids causes defective skin permeability barrier function, and neonatal lethality in ELOVL4 deficient mice. Int J Biol Sci 3(2):120–128CrossRefPubMedPubMedCentralGoogle Scholar
  9. 9.
    McMahon A, Butovich IA, Mata NL, Klein M, Ritter R 3rd, Richardson J, Birch DG, Edwards AO et al (2007) Retinal pathology and skin barrier defect in mice carrying a Stargardt disease-3 mutation in elongase of very long chain fatty acids-4. Mol Vis 13:258–272PubMedPubMedCentralGoogle Scholar
  10. 10.
    Vasireddy V, Uchida Y, Salem N Jr, Kim SY, Mandal MN, Reddy GB, Bodepudi R, Alderson NL et al (2007) Loss of functional ELOVL4 depletes very long-chain fatty acids (> or =C28) and the unique omega-O-acylceramides in skin leading to neonatal death. Hum Mol Genet 16(5):471–482. CrossRefPubMedPubMedCentralGoogle Scholar
  11. 11.
    McMahon A, Lu H, Butovich IA (2014) A role for ELOVL4 in the mouse meibomian gland and sebocyte cell biology. Invest Ophthalmol Vis Sci 55(5):2832–2840. CrossRefPubMedPubMedCentralGoogle Scholar
  12. 12.
    Brush RS, Tran JT, Henry KR, McClellan ME, Elliott MH, Mandal MN (2010) Retinal sphingolipids and their very-long-chain fatty acid-containing species. Invest Ophthalmol Vis Sci 51(9):4422–4431. CrossRefPubMedPubMedCentralGoogle Scholar
  13. 13.
    Aveldano MI (1987) A novel group of very long chain polyenoic fatty acids in dipolyunsaturated phosphatidylcholines from vertebrate retina. J Biol Chem 262(3):1172–1179PubMedGoogle Scholar
  14. 14.
    Poulos A, Johnson DW, Beckman K, White IG, Easton C (1987) Occurrence of unusual molecular species of sphingomyelin containing 28-34-carbon polyenoic fatty acids in ram spermatozoa. Biochem J 248(3):961–964. CrossRefPubMedPubMedCentralGoogle Scholar
  15. 15.
    Zanetti SR, Maldonado EN, Aveldano MI (2007) Doxorubicin affects testicular lipids with long-chain (C18-C22) and very long-chain (C24-C32) polyunsaturated fatty acids. Cancer Res 67(14):6973–6980. CrossRefPubMedGoogle Scholar
  16. 16.
    Aveldano MI (1992) Long and very long polyunsaturated fatty acids of retina and spermatozoa: the whole complement of polyenoic fatty acid series. Adv Exp Med Biol 318:231–242. CrossRefPubMedGoogle Scholar
  17. 17.
    Ozaki K, Doi H, Mitsui J, Sato N, Iikuni Y, Majima T, Yamane K, Irioka T et al (2015) A novel mutation in ELOVL4 leading to spinocerebellar ataxia (SCA) with the hot cross bun sign but lacking erythrokeratodermia: a broadened spectrum of SCA34. JAMA Neurol 72(7):797–805. CrossRefPubMedGoogle Scholar
  18. 18.
    Mir H, Raza SI, Touseef M, Memon MM, Khan MN, Jaffar S, Ahmad W (2014) A novel recessive mutation in the gene ELOVL4 causes a neuro-ichthyotic disorder with variable expressivity. BMC Med Genet 15(1):25. CrossRefPubMedPubMedCentralGoogle Scholar
  19. 19.
    Cadieux-Dion M, Turcotte-Gauthier M, Noreau A, Martin C, Meloche C, Gravel M, Drouin CA, Rouleau GA et al (2014) Expanding the clinical phenotype associated with ELOVL4 mutation: study of a large French-Canadian family with autosomal dominant spinocerebellar ataxia and erythrokeratodermia. JAMA Neurol 71(4):470–475. CrossRefPubMedGoogle Scholar
  20. 20.
    Bourassa CV, Raskin S, Serafini S, Teive HA, Dion PA, Rouleau GA (2015) A new ELOVL4 mutation in a case of spinocerebellar ataxia with erythrokeratodermia. JAMA Neurol 72(8):942–943. CrossRefPubMedGoogle Scholar
  21. 21.
    Aldahmesh MA, Mohamed JY, Alkuraya HS, Verma IC, Puri RD, Alaiya AA, Rizzo WB, Alkuraya FS (2011) Recessive mutations in ELOVL4 cause ichthyosis, intellectual disability, and spastic quadriplegia. Am J Hum Genet 89(6):745–750. CrossRefPubMedPubMedCentralGoogle Scholar
  22. 22.
    Agbaga MP (2016) Different mutations in ELOVL4 affect very long chain fatty acid biosynthesis to cause variable neurological disorders in humans. Adv Exp Med Biol 854:129–135. CrossRefPubMedGoogle Scholar
  23. 23.
    Logan S, Agbaga MP, Chan MD, Kabir N, Mandal NA, Brush RS, Anderson RE (2013) Deciphering mutant ELOVL4 activity in autosomal-dominant Stargardt macular dystrophy. Proc Natl Acad Sci U S A 110(14):5446–5451. CrossRefPubMedPubMedCentralGoogle Scholar
  24. 24.
    Sherry DM, Hopiavuori BR, Stiles MA, Rahman NS, Ozan KG, Deak F, Agbaga MP, Anderson RE (2017) Distribution of ELOVL4 in the developing and adult mouse brain. Front Neuroanat 11(38).
  25. 25.
    Mandal MN, Ambasudhan R, Wong PW, Gage PJ, Sieving PA, Ayyagari R (2004) Characterization of mouse orthologue of ELOVL4: genomic organization and spatial and temporal expression. Genomics 83(4):626–635. CrossRefPubMedGoogle Scholar
  26. 26.
    McMahon A, Butovich IA, Kedzierski W (2011) Epidermal expression of an Elovl4 transgene rescues neonatal lethality of homozygous Stargardt disease-3 mice. J Lipid Res 52(6):1128–1138. CrossRefPubMedPubMedCentralGoogle Scholar
  27. 27.
    Vassar R, Rosenberg M, Ross S, Tyner A, Fuchs E (1989) Tissue-specific and differentiation-specific expression of a human K14 keratin gene in transgenic mice. Proc Natl Acad Sci U S A 86(5):1563–1567. CrossRefPubMedPubMedCentralGoogle Scholar
  28. 28.
    Vassar R, Fuchs E (1991) Transgenic mice provide new insights into the role of TGF-alpha during epidermal development and differentiation. Genes Dev 5(5):714–727. CrossRefPubMedGoogle Scholar
  29. 29.
    Romijn HJ, van Uum JF, Breedijk I, Emmering J, Radu I, Pool CW (1999) Double immunolabeling of neuropeptides in the human hypothalamus as analyzed by confocal laser scanning fluorescence microscopy. J Histochem Cytochem 47(2):229–236. CrossRefPubMedGoogle Scholar
  30. 30.
    Ricciuti A, De Remigis A, Landek-Salgado MA, De Vincentiis L, Guaraldi F, Lupi I, Iwama S, Wand GS et al (2014) Detection of pituitary antibodies by immunofluorescence: approach and results in patients with pituitary diseases. J Clin Endocrinol Metab 99(5):1758–1766. CrossRefPubMedPubMedCentralGoogle Scholar
  31. 31.
    Bennett LD, Brush RS, Chan M, Lydic TA, Reese K, Reid GE, Busik JV, Elliott MH et al (2014) Effect of reduced retinal VLC-PUFA on rod and cone photoreceptors. Invest Ophthalmol Vis Sci 55(5):3150–3157. CrossRefPubMedPubMedCentralGoogle Scholar
  32. 32.
    Bennett LD, Hopiavuori BR, Brush RS, Chan M, Van Hook MJ, Thoreson WB, Anderson RE (2014) Examination of VLC-PUFA-deficient photoreceptor terminals. Invest Ophthalmol Vis Sci 55(7):4063–4072. CrossRefPubMedPubMedCentralGoogle Scholar
  33. 33.
    Mullen RJ, Buck CR, Smith AM (1992) NeuN, a neuronal specific nuclear protein in vertebrates. Development 116(1):201–211PubMedGoogle Scholar
  34. 34.
    Wolf HK, Buslei R, Schmidt-Kastner R, Schmidt-Kastner PK, Pietsch T, Wiestler OD, Blumcke I (1996) NeuN: a useful neuronal marker for diagnostic histopathology. J Histochem Cytochem 44(10):1167–1171. CrossRefPubMedGoogle Scholar
  35. 35.
    Chang YC, Gottlieb DI (1988) Characterization of the proteins purified with monoclonal antibodies to glutamic acid decarboxylase. J Neurosci 8(6):2123–2130PubMedGoogle Scholar
  36. 36.
    Buckley K, Kelly RB (1985) Identification of a transmembrane glycoprotein specific for secretory vesicles of neural and endocrine cells. J Cell Biol 100(4):1284–1294. CrossRefPubMedGoogle Scholar
  37. 37.
    VanGuilder HD, Brucklacher RM, Patel K, Ellis RW, Freeman WM, Barber AJ (2008) Diabetes downregulates presynaptic proteins and reduces basal synapsin I phosphorylation in rat retina. Eur J Neurosci 28(1):1–11. CrossRefPubMedGoogle Scholar
  38. 38.
    VanGuilder HD, Yan H, Farley JA, Sonntag WE, Freeman WM (2010) Aging alters the expression of neurotransmission-regulating proteins in the hippocampal synaptoproteome. J Neurochem 113(6):1577–1588. PubMedPubMedCentralGoogle Scholar
  39. 39.
    Hopiavuori BR, Masser DR, Wilkerson JL, Brush RS, Mandal NA, Anderson RE, Freeman WM (2017) Isolation of neuronal synaptic membranes by sucrose gradient centrifugation. Methods Mol Biol 1609:33–41. CrossRefPubMedGoogle Scholar
  40. 40.
    Bligh EG, Dyer WJ (1959) A rapid method of total lipid extraction and purification. Can J Biochem Physiol 37(8):911–917. CrossRefPubMedGoogle Scholar
  41. 41.
    Li F, Marchette LD, Brush RS, Elliott MH, Le YZ, Henry KA, Anderson AG, Zhao C et al (2009) DHA does not protect ELOVL4 transgenic mice from retinal degeneration. Mol Vis 15:1185–1193PubMedPubMedCentralGoogle Scholar
  42. 42.
    Laird NM, Ware JH (1982) Random-effects models for longitudinal data. Biometrics 38(4):963–974. CrossRefPubMedGoogle Scholar
  43. 43.
    Pinheiro JC, Bates DM (2000) Mixed-effects models in S and S-PLUS. Statistics and computing. Springer, New York. CrossRefGoogle Scholar
  44. 44.
    Venables WN, Ripley BD, Venables WN (2002) Modern applied statistics with S, 4th edn. Statistics and computing. Springer, New York. CrossRefGoogle Scholar
  45. 45.
    Wood SN (2006) Generalized additive models: an introduction with R. Texts in statistical science. Chapman & Hall/CRC, Boca RatonGoogle Scholar
  46. 46.
    Betz WJ, Bewick GS (1992) Optical analysis of synaptic vesicle recycling at the frog neuromuscular junction. Science 255(5041):200–203. CrossRefPubMedGoogle Scholar
  47. 47.
    Gaffield MA, Betz WJ (2006) Imaging synaptic vesicle exocytosis and endocytosis with FM dyes. Nat Protoc 1(6):2916–2921. CrossRefPubMedGoogle Scholar
  48. 48.
    Deák F, Xu Y, Chang WP, Dulubova I, Khvotchev M, Liu X, Südhof TC, Rizo J (2009) Munc18-1 binding to the neuronal SNARE complex controls synaptic vesicle priming. J Cell Biol 184(5):751–764. CrossRefPubMedPubMedCentralGoogle Scholar
  49. 49.
    Deák F, Shin OH, Kavalali ET, Südhof TC (2006) Structural determinants of synaptobrevin 2 function in synaptic vesicle fusion. J Neurosci 26(25):6668–6676. CrossRefPubMedGoogle Scholar
  50. 50.
    Deák F, Schoch S, Liu X, Südhof TC, Kavalali ET (2004) Synaptobrevin is essential for fast synaptic-vesicle endocytosis. Nat Cell Biol 6(11):1102–1108. CrossRefPubMedGoogle Scholar
  51. 51.
    Deák F, Shin OH, Tang J, Hanson P, Ubach J, Jahn R, Rizo J, Kavalali ET et al (2006) Rabphilin regulates SNARE-dependent re-priming of synaptic vesicles for fusion. EMBO J 25(12):2856–2866. CrossRefPubMedPubMedCentralGoogle Scholar
  52. 52.
    Navidhamidi M, Ghasemi M, Mehranfard N (2017) Epilepsy-associated alterations in hippocampal excitability. Rev Neurosci 28(3):307–334. CrossRefPubMedGoogle Scholar
  53. 53.
    Soussi R, Boulland JL, Bassot E, Bras H, Coulon P, Chaudhry FA, Storm-Mathisen J, Ferhat L et al (2015) Reorganization of supramammillary-hippocampal pathways in the rat pilocarpine model of temporal lobe epilepsy: evidence for axon terminal sprouting. Brain Struct Funct 220(4):2449–2468. CrossRefPubMedGoogle Scholar
  54. 54.
    Deak F, Liu X, Khvotchev M, Li G, Kavalali ET, Sugita S, Sudhof TC (2009) Alpha-latrotoxin stimulates a novel pathway of Ca2+-dependent synaptic exocytosis independent of the classical synaptic fusion machinery. J Neurosci 29(27):8639–8648. CrossRefPubMedPubMedCentralGoogle Scholar
  55. 55.
    Belanger M, Allaman I, Magistretti PJ (2011) Brain energy metabolism: focus on astrocyte-neuron metabolic cooperation. Cell Metab 14(6):724–738. CrossRefPubMedGoogle Scholar
  56. 56.
    Cash S, Yuste R (1999) Linear summation of excitatory inputs by CA1 pyramidal neurons. Neuron 22(2):383–394. CrossRefPubMedGoogle Scholar
  57. 57.
    Hao J, Wang XD, Dan Y, Poo MM, Zhang XH (2009) An arithmetic rule for spatial summation of excitatory and inhibitory inputs in pyramidal neurons. Proc Natl Acad Sci U S A 106(51):21906–21911. CrossRefPubMedPubMedCentralGoogle Scholar
  58. 58.
    Poirazi P, Brannon T, Mel BW (2003) Pyramidal neuron as two-layer neural network. Neuron 37(6):989–999. CrossRefPubMedGoogle Scholar
  59. 59.
    Poirazi P, Brannon T, Mel BW (2003) Arithmetic of subthreshold synaptic summation in a model CA1 pyramidal cell. Neuron 37(6):977–987. CrossRefPubMedGoogle Scholar
  60. 60.
    Rohrbough J, Rushton E, Palanker L, Woodruff E, Matthies HJ, Acharya U, Acharya JK, Broadie K (2004) Ceramidase regulates synaptic vesicle exocytosis and trafficking. J Neurosci 24(36):7789–7803. CrossRefPubMedPubMedCentralGoogle Scholar
  61. 61.
    El Bawab S, Usta J, Roddy P, Szulc ZM, Bielawska A, Hannun YA (2002) Substrate specificity of rat brain ceramidase. J Lipid Res 43(1):141–148PubMedGoogle Scholar
  62. 62.
    Ben Gedalya T, Loeb V, Israeli E, Altschuler Y, Selkoe DJ, Sharon R (2009) Alpha-synuclein and polyunsaturated fatty acids promote clathrin-mediated endocytosis and synaptic vesicle recycling. Traffic 10(2):218–234. CrossRefPubMedGoogle Scholar
  63. 63.
    Teixeira G, Vieira LB, Gomez MV, Guatimosim C (2012) Cholesterol as a key player in the balance of evoked and spontaneous glutamate release in rat brain cortical synaptosomes. Neurochem Int 61(7):1151–1159. CrossRefPubMedGoogle Scholar
  64. 64.
    Linetti A, Fratangeli A, Taverna E, Valnegri P, Francolini M, Cappello V, Matteoli M, Passafaro M et al (2010) Cholesterol reduction impairs exocytosis of synaptic vesicles. J Cell Sci 123(Pt 4):595–605. CrossRefPubMedGoogle Scholar
  65. 65.
    Kato K, Clark GD, Bazan NG, Zorumski CF (1994) Platelet-activating factor as a potential retrograde messenger in CA1 hippocampal long-term potentiation. Nature 367(6459):175–179. CrossRefPubMedGoogle Scholar
  66. 66.
    Izquierdo I, Fin C, Schmitz PK, Da Silva RC, Jerusalinsky D, Quillfeldt JA, Ferreira MB, Medina JH et al (1995) Memory enhancement by intrahippocampal, intraamygdala, or intraentorhinal infusion of platelet-activating factor measured in an inhibitory avoidance task. Proc Natl Acad Sci U S A 92(11):5047–5051. CrossRefPubMedPubMedCentralGoogle Scholar
  67. 67.
    Clark GD, Happel LT, Zorumski CF, Bazan NG (1992) Enhancement of hippocampal excitatory synaptic transmission by platelet-activating factor. Neuron 9(6):1211–1216. CrossRefPubMedGoogle Scholar
  68. 68.
    Chen C, Bazan NG (2005) Lipid signaling: sleep, synaptic plasticity, and neuroprotection. Prostaglandins Other Lipid Mediat 77(1–4):65–76. CrossRefPubMedGoogle Scholar

Copyright information

© The Author(s) 2017

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.

Authors and Affiliations

  • Blake R. Hopiavuori
    • 1
    • 2
  • Ferenc Deák
    • 1
    • 3
    • 4
    Email author
  • Joseph L. Wilkerson
    • 2
    • 5
  • Richard S. Brush
    • 2
    • 6
  • Nicole A. Rocha-Hopiavuori
    • 2
  • Austin R. Hopiavuori
    • 2
  • Kathryn G. Ozan
    • 2
  • Michael T. Sullivan
    • 2
  • Jonathan D. Wren
    • 7
  • Constantin Georgescu
    • 7
  • Luke Szweda
    • 8
  • Vibhudutta Awasthi
    • 1
    • 9
  • Rheal Towner
    • 1
    • 10
  • David M. Sherry
    • 1
    • 5
  • Robert E. Anderson
    • 1
    • 2
    • 4
    • 5
    • 6
    Email author
  • Martin-Paul Agbaga
    • 1
    • 2
    • 3
    • 5
    • 6
    Email author
  1. 1.Oklahoma Center for NeurosciencesUniversity of Oklahoma Health Sciences CenterOklahoma CityUSA
  2. 2.Dean McGee Eye InstituteUniversity of Oklahoma Health Sciences CenterOklahoma CityUSA
  3. 3.Harold Hamm Diabetes CenterUniversity of Oklahoma Health Sciences CenterOklahoma CityUSA
  4. 4.Reynolds Oklahoma Center on Aging, Department of Geriatric MedicineUniversity of Oklahoma Health Sciences CenterOklahoma CityUSA
  5. 5.Department of Cell BiologyUniversity of Oklahoma Health Sciences CenterOklahoma CityUSA
  6. 6.Department of OphthalmologyUniversity of Oklahoma Health Sciences CenterOklahoma CityUSA
  7. 7.Arthritis and Clinical Immunology Research ProgramOklahoma Medical Research FoundationOklahoma CityUSA
  8. 8.Department of Free Radical Biology and Aging Research ProgramOklahoma Medical Research FoundationOklahoma CityUSA
  9. 9.Department of Pharmaceutical SciencesUniversity of Oklahoma Health Sciences CenterOklahoma CityUSA
  10. 10.Department of Advanced Magnetic Resonance CenterOklahoma Medical Research FoundationOklahoma CityUSA

Personalised recommendations