The authors thank Dr. Eric C. Bolton for allowing us to use his centrifuge for fractionation and Dr. Graham H. Diering in Dr. Richard L. Huganir's lab at John's Hopkins University for providing us with the small-scale protocol for the PSD fractionation.

All experimental procedures including animal subjects have been approved by the Institutional Animals Care and Use Committee at the University of Illinois at Urbana-Champaign.
1. Maintaining a Rat Colony
<ol>
	<li>Breed Sprague-Dawley rats (see the Table of Materials) and maintain them in standard conditions with a 12-h light-dark cycle and ad libitum access to food and water.</li>
	<li>Wean the rat pups at postnatal day (P) 28 and house them in groups of 2 - 4 male or female littermates.</li>
	<li>Mark the tails of male rats with a non-toxic permanent black marker for identification.</li>
	<li>Weigh the male rats 3 times per week and record their bodyweights.</li>
</ol>
2. Preparation of an ECS Machine
<ol>
	<li>At 7:30 am, disinfect the bench in the animal preparation room and place an ECS machine (pulse generator) on the bench.</li>
	<li>Place an individual male rat weighing 200 - 250 g in a clean, empty cage with a lid. Repeat this for all male rats to be treated with ECS induction. Let the rats habituate for 30 min.</li>
	<li>While the rats are habituating in their cages, set a pulse generator for ECS induction to the frequency of 100 pulses/s, a pulse width of 0.5 ms, a shock duration of 0.5 s, and a current of 55 mA (Figure 1A).</li>
	<li>Prepare the pulse generator by pushing the &#34;RESET&#34; button and ensuring that the &#34;READY&#34; button is lit. Make sure that the ear clips are not attached to a pulse generator and then press the &#34;SHOCK&#34; button for a few seconds. 
	NOTE: At this point, the pulse generator is ready for ECS induction.</li>
	<li>Plug the ear clips into the pulse generator.</li>
</ol>
3. Induction of Acute ECS
NOTE: See Figure 1B, top panel.
<ol>
	<li>Wet the ear clips with sterile saline and ensure that they are saturated.</li>
	<li>Wet a rat&#39;s ears with sterile saline by wrapping them in saline-soaked gauze. Once they are wet, remove the gauze.</li>
	<li>Attach one clip per ear, position beyond the main cartilage band.</li>
	<li>Confirm on the ECS machine that a true loop is established; if not, an error message or a reading of &#34;1&#34; will appear on the machine.</li>
	<li>Wear a thick, non-metal glove. While holding the rat gently in a gloved hand, press the &#34;SHOCK&#34; button for a few seconds and slowly release the grip on the rat to observe the seizure. For the sham &#34;no seizure&#34; (NS) control, handle the rat identically but do not deliver the current.</li>
	<li>Disconnect the ear clips as clonus begins and record the seizure behavior according to a revised Racine&#39;s scale22 that includes &#34;mouth and facial movements&#34; (stage 1), &#34;head nodding&#34; (stage 2), &#34;forelimb clonus&#34; (stage 3), &#34;rearing with forelimb clonus&#34; (stage 4), and &#34;rearing and falling with forelimb clonus&#34; (stage 5). The seizure should last approximately 10 s; record the seizure duration using a timer.</li>
	<li>Following seizure termination, return the rat to its home cage. Monitor the rat for another 5 min to make sure of the recovery of the rat from the seizures. Keep it singly housed in the cage and return the cage to the recovery room.</li>
	<li>Repeat the ECS induction on the next rat.</li>
	<li>Monitor the rats throughout the remainder of the day and at least once in the morning and once in the afternoon the following day until they are euthanized for experiments. 
	NOTE: The ECS induction method could lead to clinical signs as an incidental side effect, which requires attention. For example, the ECS induction protocol could induce seizures that last longer than 15 s and cause unnecessary distress to the rats. In this case, terminate the seizure using diazepam (10 mg/kg, i.p.) or pentobarbital (25 - 30 mg/kg, i.p.). If the rats develop respiratory distress or severe behavioral abnormalities following seizure cessation, euthanize them by carbon dioxide inhalation followed by decapitation.</li>
</ol>
4. Induction of Chronic ECS
NOTE: See Figure 1B, bottom panel.
<ol>
	<li>Induce one ECS per day at the same time in the morning as described in steps 1 - 3, above, for seven consecutive days.</li>
	<li>Monitor the rats twice a day after they are returned to their home cages.</li>
</ol>
5. Homogenization and Fractionation of Rat Hippocampi
NOTE: See Figure 2.
<ol>
	<li>Prepare a fresh homogenization buffer (Solution A) that contains 320 mM sucrose, 5 mM sodium pyrophosphate, 1 mM EDTA, 10 mM HEPES pH 7.4, 200 nM okadaic acid, and protease inhibitors. Filter-sterilize the buffer using filters with a 0.22 &#181;m pore size for vacuum filtration and place it on ice.</li>
	<li>At a given time point following acute ECS or chronic ECS (Figure 1), euthanize the rat by CO2 inhalation for 5 - 10 min, followed by decapitation using a guillotine.</li>
	<li>Remove the brain and dissect the hippocampi on the metal plate placed on ice, as described previously23,24.</li>
	<li>Place two hippocampi from one rat onto a 30-mm tissue culture dish and mince them into small pieces using scissors.</li>
	<li>Transfer the minced hippocampi to a manual glass homogenizer using a 1 mL pipette and add 1 mL of ice-cold homogenization buffer (Solution A, step 5.1). Insert a round pestle into a glass homogenizer. While the glass homogenizer is on ice, gently and steadily stroke up and down on the pestle 10 - 15 times for 1 min, until small pieces of hippocampal tissue disappear.</li>
	<li>Transfer the homogenate to a 1.7 mL microcentrifuge tube using a 1-mL pipette and centrifuge the homogenate at 800 x g for 10 min at 4 &#176;C to separate the postnuclear supernatant (S1 fraction) from the pellet containing insoluble tissue and nuclei (P1 fraction). Transfer 50 &#181;L and 950 &#181;L of the S1 fraction to two separate, new 1.7 mL microcentrifuge tubes using a 1 mL pipette and store these tubes on ice. Save the P1 fraction pellet on ice.</li>
	<li>Centrifuge the S1 fraction (950 &#181;L) for 10 min at 13,800 x g and 4 &#176;C to separate the supernatant (S2 fraction), enriched with cytosolic-soluble proteins, and the pellet (P2 fraction), enriched with membrane-bound proteins, including synaptosomal proteins. Transfer the S2 fraction to a new 1.7 mL microcentrifuge using a 1-mL pipette and store it on ice.</li>
	<li>Resuspend the pellet (P2 fraction) in 498 &#181;L of ice-cold purified water using a 1-mL pipette. Add 2 &#181;L of 1 M HEPES (pH 7.4) using a 20 &#181;L pipette to achieve a final concentration of 4 mM HEPES (pH 7.4). Incubate at 4 &#176;C with agitation for 30 min. Store the resuspended P2 fraction on ice.</li>
	<li>Determine the protein concentration of the S1, S2, and P2 fractions using a BCA assay. Add 50 mM HEPES (pH 7.4) to each fraction to achieve a 1 mg/mL concentration and store at -80 &#176;C until use, or process the P2 fraction to isolate the PSD.</li>
</ol>
6. Isolation of the PSD from the Crude Membrane Protein (P2) Fraction
<ol>
	<li>Centrifuge the P2 fraction (500 &#181;L) for 20 min at 25,000 x g and 4 &#176;C to separate the lysed supernatant (LS2 fraction) and the lysed pellet (LP1 fraction). Transfer the LS2 fraction to a new 1.7 mL microcentrifuge tube using a 1 mL pipette and store it on ice.</li>
	<li>Resuspend the LP1 pellet in 250 &#181;L of 50 mM HEPES (pH 7.4) mixed with 250 &#181;L of 1% detergent in 1x PBS buffer using a 1 mL pipette. Incubate at 4 &#176;C with gentle agitation for 15 min.</li>
	<li>Centrifuge the resuspended LP1 pellet for 3 h at 25,000 x g and 4 &#176;C to separate the supernatant (non-PSD fraction) from the pellet (PSD fraction). Remove the supernatant to a 1.7-mL microcentrifuge tube and resuspend the PSD pellet in 100 &#181;L of 50 mM HEPES (pH 7.4) using a 200 &#181;L pipette.</li>
	<li>Determine the protein concentration of the LS2, non-PSD, and PSD fractions using a BCA assay. Add 50 mM HEPES (pH 7.4) to each fraction to achieve a 1 mg/mL concentration and store at -80 &#176;C until use. 
	NOTE: All solutions used in steps 5 - 6 (i.e., Solution A, HEPES buffer, and PBS buffer) should be made with purified water free of ionic and organic contaminants and particles.</li>
</ol>
7. Western Blotting
<ol>
	<li>Thaw each protein fraction on ice. Transfer 12 &#181;L of each fraction (S2, P2, and PSD in 1 mg/mL) to a new 1.7 mL microcentrifuge tube using a 20-&#181;L pipette.</li>
	<li>Add 3 &#181;L of 5x SDS sample buffer and incubate at 75 &#176;C for 30 min in a water bath. Cool the sample down to room temperature (RT).</li>
	<li>Load 10 &#181;L of the protein sample into each well of 4-20% gradient 15-well comb SDS-polyacrylamide gel electrophoresis (SDS-PAGE) gel using a 20 &#181;L pipette. Run the gel in the SDS-PAGE apparatus and at 80-100 V in running buffer (25 mM Tris, 190 mM glycine, and 0.1% SDS; pH 8.3). 
	NOTE: Each gel should contain protein samples from NS rats and ECS rats at different time points following acute or chronic ECS.</li>
	<li>Transfer the proteins from the SDS-PAGE gel to a polyvinyl difluoride (PVDF) membrane in the transfer apparatus at 25 - 30 V (60 mA) for 9 - 12 h in transfer buffer (25 mM Tris, 190 mM glycine, and 20% methanol; pH 8.3).</li>
	<li>Remove the PVDF membrane from the transfer apparatus and wash it in Tris-buffered saline (TBS) for 5 min on a multi-purpose rotator at RT.</li>
	<li>Block the membrane in 5% milk and 0.1% Tween-20 in TBS for 1 h. Incubate it in primary antibodies (Table 1) in washing buffer (1% milk and 0.1% Tween-20 in TBS) overnight on a multi-purpose rotator at 4 &#176;C (see the Table of Materials for dilutions).</li>
	<li>Wash the membrane 4 times for 10 min each in wash buffer and then incubate it with horseradish peroxidase (HRP)-conjugated secondary antibodies in washing buffer for 1 h on a multi-purpose rotator at RT.</li>
	<li>Wash the membrane 4 times for 10 min each in wash buffer and then with TBS for 5 min.</li>
	<li>Incubate the membrane with enhanced chemifluorescence substrate for 1 min and expose it to X-ray film. Develop the exposed film with a film processor.</li>
</ol>
8. Quantification of Western Blots
<ol>
	<li>Scan the Western blot as a TIFF file and save this file to the computer.</li>
	<li>Open the Western blot file in the ImageJ program as a grayscale image, under &#34;File,&#34; &#34;Open image,&#34; right arrow &#34;gray-scale.&#34;</li>
	<li>Choose the rectangular selection tool from the ImageJ toolbar and draw a rectangle that covers a single Western blot band of a protein of interest.</li>
	<li>Under &#34;Analyze,&#34; hit &#34;Measure&#34; to obtain the area and the mean density of a selected band.</li>
	<li>Move the rectangle to a background area without changing its size and shape. Repeat step 8.4 to the area and the mean density of a background.</li>
	<li>Subtract the mean density value of a background band from that of a Western blot band, giving the background-subtracted band density of the protein of interest.</li>
	<li>Repeat steps 8.2 - 8.6 for all Western blot bands of interest.</li>
	<li>Divide the background-subtracted band density of the protein of interest by the background-subtracted band density of a housekeeping gene product, such as &#945;-Tubulin; this step yields the normalized value of the protein of interest.</li>
</ol>

The authors declare that they have no competing financial interests.

Here, we describe an ECS induction method in rats that elicits the global stimulation of neuronal activity in their hippocampi. ECS is an animal model of electroconvulsive therapy, which is clinically used to treat drug refractory depressive disorders in humans1,2,3. Despite use of electroconvulsive therapy to treat severe depression, the precise underlying mechanism remains unclear. Because ECS induces anti-depressant-like behaviors in rodents and stimulates hippocampal neurogenesis4,32, ECS has been extensively used to investigate if new adult-born neurons in the dentate gyrus of the hippocampus contribute to anti-depressant behavior5,32.
ECS induces mild to severe generalized tonic-clonic seizures in rodents upon current delivery through stereotaxically implanted electrodes, corneal electrodes, or ear-clip electrodes33,34. EEG recordings in patients have revealed that bilateral electrical stimulation causes more prominent and longer generalized seizures than unilateral stimulation does35,36. In our ECS induction method, tonic-clonic seizures are induced by current delivery through noninvasive ear-clip electrodes attached to both ears, mimicking seizures in humans evoked by bilateral stimulation36.&#160;Although we haven&#8217;t checked the efficacy of ECS in the rats to which sedation or anesthesia is applied, it is feasible that giving anesthetic drugs to the rats could reduce the degree of seizures induced by electrical stimulation, which might be due to the fact that anesthesia state is physiologically associated with enhanced inhibitory and dampened excitatory tone in the brain network. In addition, the critical step in the ECS induction method is to experimentally dial the current intensity to elicit stage 4 - 5 generalized tonic- clonic seizures based on the age, weight, and the species of rodent. &#160;Our ECS induction method has been optimized for inducing stage 4 - 5 seizures within a few seconds in awake male Sprague-Dawley rats weighing 200 - 250 g. If the rats under anesthesia state are used for ECS induction, the intensity, duration, and frequency of delivering current should be modified for successful induction of seizure ranging from stage 4 to 5.&#160;
ECS also offers the advantage of stimulating hyperactivity in neurons and causing acute transient seizures with very low mortality33, in contrast to chemoconvulsants, including pilocarpine and kainite, which induce status epilepticus and cause chronic manifestation of spontaneous recurrent seizures and severe histological alterations37,38. Although ECS has been routinely utilized to screen anti-epileptic drugs33,34, acute ECS and chronic ECS do not result in the generation of chronic epilepsy and thus cannot be used in an animal model to study epileptogenesis. Instead, ECS has been widely employed to examine the extent to which the broad elevation of brain activity alters expression and/or posttranslational modifications of synaptic proteins in vivo, which contribute to persistent changes in synaptic strength and structures (Figure 3 and Figure 4)10,40. In this study, we only used male rats to exclude the unexpected effects of the estrus cycle phase of female rats on the amount of PSD protein after ECS. However, it was observed that there is no sex difference in the scaffolding proteins, including PSD-95 and SAP102 in the PSD region of the frontal cortex and hippocampus39, implying that hormonal changes governing estrus cycle might not affect the basal amount of PSD proteins.
Multiple methods have been employed to examine the extent to which ECS induces changes in neurogenesis, synaptogenesis, and synaptic plasticity5,6,7,8,9,11,40. Electrophysiological recordings of excitatory postsynaptic current (EPSC) are widely used to detect the changes in the synaptic strength of glutamatergic excitatory synapses21. For example, miniature EPSC recordings have revealed the homeostatic downscaling of excitatory synaptic strength in the cortical pyramidal neurons of layers II-III of mice following acute ECS41. However, the identification of synaptic proteins that contribute to ECS-induced synaptic plasticity is challenging because electrophysiological recordings must be paired with the genetic knockout or knock-down of specific candidate synaptic proteins. Changes in the level of glutamate receptors at the postsynaptic membrane and synaptic proteins enriched in the PSD regulate the strength and efficacy of excitatory synaptic transmission17,18,25. Although immunohistochemistry can be used to examine ECS-induced changes in the expression of synaptic proteins, this technique can examine only 1 - 2&#160; candidate synaptic proteins at a time and requires well-validated antibodies that specifically recognize them without causing non-specific staining.
The subcellular fractionation of brain tissue in combination with Western blotting offers advantages over electrophysiology and immunohistochemistry in identifying synaptic proteins that are altered by ECS. The subcellular fractionation of brain tissue is a rapid and crude biochemical method to separate soluble cytosolic proteins (S2 fraction) from crude membranes (P2 fraction), including ER and Golgi membranes, membrane-bound organelles, plasma membranes, and synaptic terminal membranes that reseal to form synaptosomes42,43,44. The PSD fraction can be further isolated from the P2 fraction to enrich the synaptic proteins42,43,44. The unbiased proteomic analysis of the PSD fraction could identify all PSD proteins whose levels are altered by ECS. Western blotting can be performed rapidly to examine the expression changes of the PSD proteins, which can be easily identified from non-specific bands.
The previous method of brain fractionation requires a large amount of rodent brain tissue42,43,44, making this technique challenging for use when examining soluble or membrane proteins from an individual rodent brain or a specific brain region from a single brain. There is an increasing demand to quantitatively compare the proteome from one brain region to another and from a control animal to a transgenic animal or an animal that has undergone a specific treatment. Hence, we have revised and optimized the traditional brain fractionation method to isolate crude soluble and membrane fractions from two hippocampi of a single rat. Our small-scale crude fractionation protocol successfully isolated crude P2 membrane fractions from cytosolic S2 soluble fractions, as indicated by the lack of cytoplasmic protein &#945;-tubulin in the P2 fractions, whereas membrane-bound PSD95 was detected in the P2 but not S2 fractions (Figure 3A and Figure 4A). Using the method described here, we have quantitatively shown that acute ECS significantly increases STEP61 expression and decreases tyrosine phosphorylation of its substrates, GluN2B and the extracellular signal-regulated kinase 1/2 in the crude membrane P2 fraction of rat hippocampi at 48 h following acute ECS10.
Unexpectedly, the S2 fractions contained synaptophysin; STEP61; and, to a much lesser extent, GluA2 (Figure 3A and Figure 4A). STEP61 is a glycosylated integral membrane protein26 associated with the endoplasmic reticulum (ER) and PSD45. It is possible that the centrifugation to isolate the crude membrane pellet (P2 fraction) might not have been sufficient to pellet all synaptic vesicles containing synaptosomes, as well as endosomes and lysosomes containing GluA2 and STEP61. Nonetheless, clear enrichment of GluN2B, GluA2, and PSD95 and the lack of &#945;-tubulin in the P2 fractions indicate that our fractionation protocol can enrich membrane-bound proteins and transmembrane proteins that are not associated with synaptic vesicles and endosomes in the crude membrane P2 fraction.
Although the crude membrane P2 fraction contains synaptosomes, one limitation of examining activity-dependent alterations of synaptic proteins in the P2 fraction is that the exact location of their changes cannot be determined. If synaptic proteins enriched in the PSD were to be determined, then further biochemical fractionation can be used to isolate the PSD. The previous method of PSD fractionation requires a large amount of rodent brain tissue (i.e., 10 - 20 rodent brains) and sucrose gradients42,43,44. Because this traditional method is inadequate to isolate a sufficient amount of the PSD fraction from two hippocampi of a single rat, we have adapted a simpler method that directly isolates the PSD fraction, without a sucrose gradient20,21. This method yields about 30 - 50 &#181;g of the PSD protein, sufficient for several biochemical assays, including Western blotting. Our method enriches PSD95, GluN2B, and GluA2, which are known to be concentrated in the PSD fraction, and detects changes in GluN2B expression in PSD fraction following chronic ECS induction (Figure 3 and Figure 4).
Here, our quantitative Western blot analysis revealed no significant change in GluA2 expression in the P2 and PSD fractions at 3 h and 24 h following acute ECS (Figure 3C). The GluN2B expression was unaltered in the P2 fraction but displayed an increasing trend in the PSD fraction at 3 h and 24 h after acute ECS (Figure 3B), suggesting the possible differential regulation of synaptic versus extrasynaptic GluN2B-containing NMDA receptors. We also observed that GluN2B expression displayed a decreasing trend in the P2 fraction after chronic ECS and was significantly reduced in the PSD fraction at 24 and 96 h following chronic ECS (Figure 4B). Though highly speculative, such removal of GluN2B from the PSD following repetitive induction of ECS may be mediated by multiple mechanisms, including direct internalization from the PSD membrane or lateral diffusion to extrasynaptic sites. Considering our previous report that prolonged enhancement of neuronal activity markedly increases STEP61 expression and reduces Tyr-phosphorylation of GluN2B in the P2 fractions of cultured hippocampal neurons46, our findings suggest that a decrease in GluN2B expression in the P2 and the PSD fractions after chronic ECS may be likely due to enhanced STEP61 expression and the subsequent removal of GluN2B from the extrasynaptic membrane.
In summary, we have demonstrated that our small-scale PSD fractionation method, in combination with an ECS induction protocol, allows us to differentiate in vivo the activity-dependent regulation of glutamate receptors at the postsynaptic membrane versus total plasma membranes, including the extrasynaptic membranes. This protocol can easily be applied to any synaptic proteins at excitatory synapses and can be modified for other rodent hippocampi or other brain regions by adjusting the volume of each solution based on the tissue weight. Thus, our small-scale PSD fractionation method is versatile and can be adopted for future applications to examine the in vivo changes in the postsynaptic proteins in each animal upon genetic, pharmacological, or mechanical treatment.

Electroconvulsive therapy has been used to treat patients with major depressive disorders, including severe drug-resistant depression, bipolar depression, Parkinson&#39;s diseases, and schizophrenia1,2. In this therapy, seizure is generated by electrical stimulus delivered to the head of anesthetized patients via epicranial electrodes1,2,3. Repetitive administration of ECS has been clinically beneficial to drug-resistant depressive disorders1,2,3. However, the exact mechanism underlying the long-term efficacy of the antidepressant effect in humans has remained elusive. ECS is an animal model of electroconvulsive therapy and is widely used to investigate its therapeutic mechanism. In rodents, both acute ECS and chronic ECS treatment promote adult neurogenesis in the hippocampi and reorganize the neural network4,5, which is likely to contribute to improvements in cognitive flexibility. Furthermore, global elevation of brain activity by ECS alters the abundance of transcripts, such as a brain derived neurotropic factor6, and multiple proteins, including metabotropic glutamate receptor 17 and the N-methyl-D-aspartate (NMDA) type glutamate receptor subunits7. These changes are involved in mediating long-term modification of synapse number, structure, and strength in the hippocampus7,8,9.
In ECS models, electrical stimulation is delivered to rodents via stereotaxically implanted electrodes, corneal electrodes, or ear electrodes to evoke generalized tonic-clonic seizures10,11. Stereotaxic implantation of electrodes involves brain surgery and requires significant time to improve the experimenter&#39;s surgical skills to minimize injury. Less invasive corneal electrodes could cause corneal abrasion and dryness and require anesthesia. The use of ear-clip electrodes bypasses these limitations because they can be used on rodents without surgery or anesthesia and cause minimal injury. Indeed, we found that current delivered to awake rats via ear-clip electrodes reliably induces stage 4-5 tonic-clonic seizures and alters synaptic proteins in their hippocampi10.
To examine the ECS-induced abundance of synaptic proteins in the specific brain regions of the rodents, it is important to choose the experimental methods that are most suitable for their detection and quantification. Subcellular fractionation of the brain allows for the crude isolation of soluble cytosolic proteins; membrane proteins; organelle-bounds proteins; and even proteins in special subcellular structures, such as the PSD12,13,14. The PSD is a dense and well-organized subcellular domain in neurons in which synaptic proteins are highly concentrated at and near the postsynaptic membrane12,13,15. The isolation of the PSD is useful for the study of synaptic proteins enriched at the PSD, since dynamic changes in the abundance and function of postsynaptic glutamate receptors, scaffolding proteins, and signal transduction proteins in the PSD12,15,16,17 are correlated with synaptic plasticity and the synaptopathy observed in several neurological disorders17,18. A previous subcellular fractionation method used to purify the PSD involved the isolation of the detergent-insoluble fraction from the crude membrane fraction of the brain by the differential centrifugation of sucrose gradients14,19. The major challenge with this traditional method is that it requires large amounts of rodent brains14,19. Preparation of 10 - 20 rodents to isolate the PSD fraction per treatment requires extensive cost and time investment and is not practically feasible if there are many treatments.
To overcome this challenge, we have adapted a simpler method that directly isolates the PSD fraction, without sucrose gradient centrifugation20,21, and revised it to be applicable to PSD isolation from the hippocampi of a single rat brain.Our small-scale PSD fractionation method yields about 30 - 50 &#181;g of the PSD proteins from 2 hippocampi, sufficient for use in several biochemical assays, including immunoprecipitation and Western blotting. Western blotting demonstrates the success of our method for isolating the PSD by revealing the enrichment of postsynaptic density protein 95 (PSD-95) and the exclusion of presynaptic marker synaptophysin and soluble cytoplasmic protein &#945;-tubulin. Our ECS induction and small-scale PSD fractionation methods are easily adaptable to other rodent brain regions and provide a relatively simple and reliable way to evaluate the effects of ECS on the expression of PSD proteins.

<table><tbody><tr><td>Spargue-Dawley rat</td><td>Charles River Laboratories</td><td></td><td>ECS supplies</td></tr><tr><td>A pulse generator</td><td>Ugo Bsile, Comerio, Italy</td><td>57800</td><td>ECS supplies</td></tr><tr><td>MilliQ water purifying system</td><td>EMD Millipore</td><td>Z00Q0VWW</td><td>Subcellular fractionation supplies</td></tr><tr><td>Sucrose</td><td>Em science</td><td>SX 1075-3</td><td>Subcellular fractionation supplies</td></tr><tr><td>Na&lt;sub&gt;4&lt;/sub&gt;O&lt;sub&gt;7&lt;/sub&gt;P&lt;sub&gt;2&lt;/sub&gt;</td><td>SIGMA-ALDRICH</td><td>221368</td><td>Subcellular fractionation supplies</td></tr><tr><td>Ethylenediaminetetraacetic acid (EDTA)</td><td>SIGMA-ALDRICH</td><td>E9884</td><td>Subcellular fractionation supplies</td></tr><tr><td>HEPES</td><td>SIGMA-ALDRICH</td><td>H0527</td><td>Subcellular fractionation supplies</td></tr><tr><td>Okadaic acid</td><td>TOCRIS</td><td>1136</td><td>Subcellular fractionation supplies</td></tr><tr><td>Halt Protease Inhibitor</td><td>Thermo Scientific</td><td>78429</td><td>Subcellular fractionation supplies</td></tr><tr><td>NaVO&lt;sub&gt;3&lt;/sub&gt;</td><td>SIGMA-ALDRICH</td><td>72060</td><td>Subcellular fractionation supplies</td></tr><tr><td>EMD Millipore Sterito Sterile Vacuum Bottle-Top Filters</td><td>Fisher Scientific</td><td>SCGPS05RE</td><td>Subcellular fractionation supplies</td></tr><tr><td>Iris Scissors</td><td>WPI (World Precision Instruments)</td><td>500216-G</td><td>Subcellular fractionation supplies</td></tr><tr><td>30 mm tissue culture dish</td><td>Fisher Scientific</td><td>08-772B</td><td>Subcellular fractionation supplies</td></tr><tr><td>Glass homogenizer and a Teflon pestle</td><td>VWR</td><td>89026-384</td><td>Subcellular fractionation supplies</td></tr><tr><td>1.7 mL microcentrifuge tube</td><td>DENVILLE SCIENTIFIC INC.&amp;nbsp;</td><td>C2170 (1001002)</td><td>Subcellular fractionation supplies</td></tr><tr><td>Sorvall Legend XT/XF Centrifuge&amp;nbsp;</td><td>Thermo Fisher</td><td>75004521</td><td>Subcellular fractionation supplies</td></tr><tr><td>Pierce BCA Protein Assay Reagent A, 500 mL</td><td>Thermo Fisher</td><td>#23228</td><td>Western blot supplies</td></tr><tr><td>Pierce BCA Protein Assay Reagent B, 25 mL</td><td>Thermo Fisher</td><td>#1859078</td><td>Western blot supplies</td></tr><tr><td>SDS-polyacrylamide gel (SDS-PAGE)</td><td>BIO-RAD</td><td>#4561086S</td><td>Western blot supplies</td></tr><tr><td>Running Buffer</td><td>Made in the lab</td><td></td><td>Western blot supplies.&amp;nbsp;</td></tr><tr><td>Mini-PROTEAN Tetra Vertical Electrophorsis Cell for MiniPrecast Gels, 4-gel</td><td>BIO-RAD</td><td>#1658004</td><td>Western blot supplies</td></tr><tr><td>Polyvinyl difluoride (PVDF) membrane&amp;nbsp;</td><td>Milipore</td><td>IPVH00010</td><td>Western blot supplies</td></tr><tr><td>Transfer Buffer</td><td>Made in the lab</td><td></td><td>Western blot supplies.&amp;nbsp;</td></tr><tr><td>Tris-base</td><td>Fisher Scientific</td><td>BP152-1</td><td>Western blot supplies</td></tr><tr><td>Glycine</td><td>Fisher Scientific</td><td>BP381-5</td><td>Western blot supplies</td></tr><tr><td>Sodium dodecyl sulfate</td><td>SIGMA-ALDRICH</td><td>436143</td><td>Western blot supplies</td></tr><tr><td>Methanol&amp;nbsp;</td><td>Fisher Scientific</td><td>A454-4</td><td>Western blot supplies</td></tr><tr><td>Triton X-100</td><td>Fisher Scientific</td><td>BP151-500</td><td>detergent for PSD isolation</td></tr><tr><td>Mini Trans-Blot Module&amp;nbsp;</td><td>BIO-RAD</td><td>#1703935</td><td>Western blot supplies</td></tr><tr><td>Nonfat instant dry milk</td><td>Great value</td><td></td><td>Western blot supplies</td></tr><tr><td>Multi-purposee rotator&amp;nbsp;</td><td>Thermo Scientific</td><td>Model-2314</td><td>Western blot supplies</td></tr><tr><td>Hyblot CL Autoradiography Film</td><td>DENVILLE SCIENTIFIC INC.&amp;nbsp;</td><td>E3018 (1001365)</td><td>Western blot supplies</td></tr><tr><td>Enhanced chemifluorescence substrate&amp;nbsp;</td><td>Thermo Scientific</td><td>32106</td><td>Western blot supplies</td></tr><tr><td>a Konica SRX-101A film processor</td><td>KONICA MINOLTA</td><td>SRX-101A</td><td>Western blot supplies</td></tr><tr><td>&lt;strong&gt;Name of Antibody&lt;/strong&gt;</td><td></td><td></td><td></td></tr><tr><td>PSD-95</td><td>Cell Signaling</td><td>#2507</td><td>Antibody dilution = 1:500 - 1,000, time = 9 - 12 h, Reaction Temperature = 4 &amp;deg;C, Host Species = Rabbit</td></tr><tr><td>Synaptophysin</td><td>Cell Signaling</td><td>#4329</td><td>Antibody dilution = 1:500 - 1,000, time = 9 - 12 h, Reaction Temperature = 4 &amp;deg;C, Host Species = Rabbit</td></tr><tr><td>alpha-Tubulin</td><td>Santacruz</td><td>SC-5286</td><td>Antibody dilution = 1:500 - 1,000, time = 9 - 12 h, Reaction Temperature = 4 &amp;deg;C, Host Species = Mouse</td></tr><tr><td>GluN2B</td><td>Neuromab</td><td>75-097</td><td>Antibody dilution = 1:500 - 1,000, time = 9 - 12 h, Reaction Temperature = 4 &amp;deg;C, Host Species = Mouse</td></tr><tr><td>GluA2</td><td>Sigma-aldrich</td><td>Sab 4501295</td><td>Antibody dilution = 1:500 - 1,000, time = 9 - 12 h, Reaction Temperature = 4 &amp;deg;C, Host Species = Rabbit</td></tr><tr><td>STEP</td><td>Santacruz</td><td>SC-23892</td><td>Antibody dilution = 1:200 - 500, time = 9 - 12 h, Reaction Temperature = 4 &amp;deg;C, Host Species = Mouse</td></tr><tr><td>Peroxidas AffiniPure Donkey Anti-Mouse IgG (H+L)</td><td>Jackson ImmunoReserch laboratory</td><td>715-035-150</td><td>Antibody dilution = 1:2,000-5,000, time = 1 h, Reaction Temperature = RT, Host Species = Donkey</td></tr><tr><td>Peroxidas AffiniPure Donkey Anti-Rabbit IgG (H+L)</td><td>Jackson ImmunoReserch laboratory</td><td>711-035-152</td><td>Antibody dilution = 1:2,000-5,000, time = 1 h, Reaction Temperature = RT, Host Species = Donkey</td></tr></tbody></table>

electroconvulsive seizures in rats and fractionation of their hippocampi to examine seizure-induced changes in postsynaptic density proteins

Electroconvulsive seizure (ECS) is an experimental animal model of electroconvulsive therapy, the most effective treatment for severe depression. ECS induces generalized tonic-clonic seizures with low mortality and neuronal death and is a widely-used model to screen anti-epileptic drugs. Here, we describe an ECS induction method in which a brief 55-mA current is delivered for 0.5 s to male rats 200 - 250 g in weight via ear-clip electrodes. Such bilateral stimulation produced stage 4 - 5 clonic seizures that lasted about 10 s. After the cessation of acute or chronic ECS, most rats recovered to be behaviorally indistinguishable from sham &#34;no seizure&#34; rats. Because ECS globally elevates brain activity, it has also been used to examine activity-dependent alterations of synaptic proteins and their effects on synaptic strength using multiple methods. In particular, subcellular fractionation of the postsynaptic density (PSD) in combination with Western blotting allows for the quantitative determination of the abundance of synaptic proteins at this specialized synaptic structure. In contrast to a previous fractionation method that requires large amount of rodent brains, we describe here a small-scale fractionation method to isolate the PSD from the hippocampi of a single rat, without sucrose gradient centrifugation. Using this method, we show that the isolated PSD fraction contains postsynaptic membrane proteins, including PSD95, GluN2B, and GluA2. Presynaptic marker synaptophysin and soluble cytoplasmic protein &#945;-tubulin were excluded from the PSD fraction, demonstrating successful PSD isolation. Furthermore, chronic ECS decreased GluN2B expression in the PSD, indicating that our small-scale PSD fractionation method can be applied to detect the changes in hippocampal PSD proteins from a single rat after genetic, pharmacological, or mechanical treatments.

Using the detailed procedure presented here, one electrical shock (55 mA, 100 pulses/s for 0.5 s) delivered via ear-clip electrodes induced nonrecurring stage 4-5 tonic-clonic seizures in rats (Figure 1A-B). A total 8 of rats received acute ECS induction and displayed stage 4-5 tonic-clonic seizures. The seizures lasted about 10 s, and all rats recovered within 1 - 2 min of seizure cessation. Sham &#34;no seizure&#34; rats did not receive an electric shock and therefore did not display seizures. A total of 4 sham rats were used. For chronic ECS induction, the rats received one electric shock per day for 7 consecutive days and displayed stage 4-5 tonic-clonic seizures upon each electric shock (Figure 1A-B). A total 8 of rats received chronic ECS induction and a total of 4 sham rats were used as &#34;no seizure&#34; rats. Although most rats that received chronic ECS were behaviorally indistinguishable from sham &#34;no seizure&#34; rats, a few developed body tremors and reduced exploratory activity by the 7th electric shock.
To examine if ECS-induced global elevation of activity alters protein expression in the hippocampi, rats were sacrificed at 3 h and 24 h after acute ECS and at 24 h and 96 h after the final ECS in chronic ECS treatment (Figure 1B). Two hippocampi from each rat were rapidly dissected and subjected to our optimized small-scale fractionation protocol (Figure 2). The initial homogenate of two hippocampi free of insoluble tissue and nuclei (S1 fraction) was re-centrifuged at 13,800 x g for 10 min to separate the supernatant containing soluble cytoplasmic proteins (S2 fraction) from the crude membrane pellet containing synaptosomes (P2 fraction) (Figure 2). Our Western blot detected cytoplasmic protein &#945;-tubulin in the S2 fractions, but not the P2 fractions, of the hippocampi from rats treated with acute and chronic ECS (Figure 3 and Figure 4), demonstrating the successful fractionation of cytosolic soluble proteins from crude membrane pellets.
PSD95 is a member of the membrane-associated guanylate kinase (MAGUK) family and a core component of PSD12,18,25. PSD95 and NMDA receptor subunit GluN2B were detected exclusively in the P2 fractions, but not the S2 fractions (Figure 3 and Figure 4). Stronger expression of another glutamatergic &#945;-amino-3-hydroxy-5-methyl-4-isoxazolepropionic acid (AMPA) receptor subunit GluA2 was detected in the P2 fractions compared to the S2 fractions in the hippocampi (Figure 3 and Figure 4), indicating that postsynaptic membrane proteins are enriched in the crude membrane P2 fraction pellets. Interestingly, synaptic vesicle protein synaptophysin and integral membrane protein Striatal Enriched Tyrosine Phosphatase 61 (STEP61)26 were detected equally in the S2 and P2 fractions (Figure 3 and Figure 4). Considering the small size of synaptic vesicles-with an average diameter of 39 nm27 and endosomes, the centrifugation to isolate the crude membrane pellet (P2 fraction) might not have been sufficient to pellet all synaptic vesicles and endosomes. These results together indicate that our crude fractionation protocol can enrich membrane-bound proteins and transmembrane proteins that are not associated with synaptic vesicles and possibly with endosomes in the crude membrane P2 fraction.
To examine if ECS-induced global elevation of activity alters the expression of postsynaptic proteins in the hippocampi, the crude membrane P2 fraction was lysed in ice-cold water, resuspended in HEPES buffer, and centrifuged at 25,000 x g for 20 min to isolate the lysed pellet (LP1) (Figure 2). The LP1 pellet was resuspended in HEPES buffer containing 1% Triton X-100 detergent and centrifuged at 25,000 x g over 3 h to obtain the PSD pellet (Figure 2). The subsequent Western blot of the PSD fractions detected PSD95, GluN2B, and GluA2 (Figure 3 and Figure 4), which are known postsynaptic proteins17,25,28. However, the PSD fractions lacked &#945;-tubulin and, importantly, presynaptic marker synaptophysin (Figure 3 and Figure 4). STEP61, which dephosphorylates GluN2B and GluA2 and acts as their negative regulator29,30,31, was not found in the PSD fractions (Figure 3 and Figure 4), consistent with the recent report demonstrating the synaptic exclusion of STEP61, mediated by PSD95 enriched in the PSD26. Altogether, these results indicate that our small-scale fractionation method successfully isolates PSD proteins from the crude membrane P2 fraction.
The quantification of Western blotting revealed that GluN2B expression was unaltered in the P2 fraction but displayed an increasing trend in the PSD fraction at 3 h and 24 h after acute ECS (n = 4) (Figure 3B). GluA2 expression was not changed in both the P2 and PSD fractions at 3 h and 24 h following acute ECS (Figure 3C). At 24 h and 96 h after chronic ECS, GluN2B expression displayed a decreasing trend in the P2 fraction and was significantly reduced in the PSD fraction (24 h: p &#60;0.05, n = 4; 48 h: p &#60;0.01, n = 4) (Figure 4B). In contrast, chronic ECS did not affect GluA2 expression in the P2 and PSD fractions (n = 4) (Figure 4C).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/56016/56016fig1.jpg" /> 
Figure 1: Schema for the Induction of Acute ECS and Chronic ECS. (A) A rat was connected to a pulse generator via ear-clip electrodes and an electrical shock (55 mA, 100 pulses/s for 0.5 s) was applied to elicit stage 4-5 tonic-clonic seizures. (B) Acute ECS was induced by one electric shock. Chronic ECS was elicited by one electric shock per day for 7 consecutive days. The time points shown represent the duration following the induction of acute ECS or the last ECS for chronic ECS induction prior to dissection of the hippocampi. Sham &#34;no seizure&#34; (NS) control rats were handled identically but did not receive an electrical shock. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56016/56016fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/56016/56016fig2.jpg" /> 
Figure 2: Workflow of Subcellular Fractionation to Isolate the S2, P2, and PSD Fractions from the Hippocampi of a Single Rat. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56016/56016fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/56016/56016fig3.jpg" /> 
Figure 3: Examination of Synaptic Proteins in Hippocampal S2, P2, and PSD Fractions from the Rats that Received NS or Acute ECS. (A) Representative Western blots show the protein expression of NMDA receptor subunit GluN2B, AMPA receptor GluA2, and STEP61 in the S2, P2, and PSD fractions from the hippocampi of sham &#34;no seizure&#34; (NS) rats and rats that received acute ECS. The cytoplasmic-soluble protein &#945;-tubulin is enriched in the S2 fraction. Synaptophysin is a presynaptic vesicle protein and is enriched in the crude membrane P2 fraction, but not in the PSD fraction. PSD-95 is enriched in both the P2 and PSD fractions. (B-C) Quantification of GluN2B (B) and GluA2 (C) in the P2 and PSD fractions at 3 and 24 h after acute ECS (n = 4 rats per time point). GluN2B and GluA2 expression in the P2 fraction was normalized to &#945;-Tubulin in the S2 fraction. GluN2B and GluA2 expression in the PSD fraction was normalized to PSD-95 in the PSD fraction. The data are presented as the percent &#177; SEM. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56016/56016fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/56016/56016fig4.jpg" /> 
Figure 4: Examination of Synaptic Proteins in Hippocampal S2, P2, and PSD Fractions from the Rats that Received NS or Chronic ECS. Representative Western blots of &#945;-tubulin; synaptophysin; STEP61; and postsynaptic proteins, including PSD95, GluN2B, and GluA2, in the S2, P2, and PSD fractions from the hippocampi of sham &#34;no seizure&#34; (NS) rats and rats that received chronic ECS. The cytoplasmic-soluble protein &#945;-tubulin is enriched in the S2 fraction. Synaptophysin is a presynaptic vesicle protein and is enriched in the crude membrane P2 fraction, but not in the PSD fraction. PSD-95 is enriched in both the P2 and PSD fractions. (B-C) Quantification of GluN2B (B) and GluA2 (C) in the P2 and PSD fractions at 24 and 96 h after chronic ECS (n = 4 rats per time point). GluN2B and GluA2 expression in the P2 fraction was normalized to the &#945;-Tubulin in the S2 fraction. GluN2B and GluA2 expression in the PSD fraction was normalized to PSD-95 in the PSD fraction. The data are presented as percent &#177; SEM; *p &#60;0.05, **p &#60;0.01 compared with control (ANOVA and Tukey&#39;s post-hoc test). <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/56016/56016fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table fo:keep-together.within-page="1">
	<tbody>
		<tr>
			<td>Fraction</td>
			<td>Protein fraction</td>
			<td>Protein marker</td>
		</tr>
		<tr>
			<td>P1</td>
			<td>Nuclear</td>
			<td>Histon H1</td>
		</tr>
		<tr>
			<td>S1</td>
			<td>Cytosol/membrances&#160;</td>
			<td>a-tubulin (cytoskeleton) and GAPDH (cytosol)</td>
		</tr>
		<tr>
			<td>P2&#160;</td>
			<td>Crude synaptosomes</td>
			<td>AMPA and NMDA receptor subunits</td>
		</tr>
		<tr>
			<td>S2</td>
			<td>Cytosol/light membrances&#160;</td>
			<td>GAPDH (cytosol) and LAMP1 (lysosome)</td>
		</tr>
		<tr>
			<td>Synaptosomal membrane&#160;</td>
			<td>Synaptosome/mitochondria</td>
			<td>AMPA and NMDAR receptor subunits, Synaptophysin (presynaptic marker)</td>
		</tr>
		<tr>
			<td>PSD</td>
			<td>PSD</td>
			<td>AMPA and NMDA receptor subunits, PSD95, PICK1, CaMKII</td>
		</tr>
	</tbody>
</table>
Table 1: List of Protein Markers and Antibodies to Distinguish Subcellular Fractions.

Watch this Scientific Journal Video about Electroconvulsive Seizures in Rats and Fractionation of Their Hippocampi to Examine Seizure-induced Changes in Postsynaptic Density Proteins at JoVE.com

Electroconvulsive Seizures in Rats and Fractionation of Their Hippocampi to Examine Seizure-induced Changes in Postsynaptic Density Proteins

Electroconvulsive seizure (ECS) is an experimental animal model of electroconvulsive therapy for severe depression. ECS globally stimulates activity in the hippocampus, leading to synaptogenesis and synaptic plasticity. Here, we describe methods for ECS induction in rats and for subcellular fractionation of their hippocampi to examine seizure-induced changes in synaptic proteins.

Electroconvulsive seizure (ECS) is an experimental animal model of electroconvulsive therapy, the most effective treatment for severe depression. ECS ...

electroconvulsive-seizures-rats-fractionation-their-hippocampi-to

Nanyang Technological University

Research

JoVE Journal

Neuroscience

12.0K Views.  University of Illinois at Urbana-Champaign. Elektroconvulsietherapie overname (ECS) is een experimentele diermodel van elektroconvulsieve therapie voor ernstige depressie. ECS stimuleert wereldwijd activiteit in de hippocampus, wat leidt tot synaptogenese en synaptische plasticiteit. Hier beschrijven we methoden voor ECS inductie bij ratten en voor subcellular versplintering van hun hippocampi te onderzoeken van inbeslagneming-geïnduceerde veranderingen in synaptic eiwitten.

Video: Electroconvulsive Seizures in Rats and Fractionation of Their Hippocampi to Examine Seizure-induced Changes in Postsynaptic Density Proteins

Preparation of Acute Hippocampal Slices from Rats and Transgenic Mice for the Study of Synaptic Alterations during Aging and Amyloid Pathology

The rodent hippocampal slice preparation is perhaps the most broadly used tool for investigating mammalian synaptic function and plasticity. The hippocampus can be extracted quickly and easily from rats and mice and slices remain viable for hours in oxygenated artificial cerebrospinal fluid. Moreover, basic electrophysisologic techniques are easily applied to the investigation of synaptic function in hippocampal slices and have provided some of the best biomarkers for cognitive impairments. The hippocampal slice is especially popular for the study of synaptic plasticity mechanisms involved in learning and memory. Changes in the induction of long-term potentiation and depression (LTP and LTD) of synaptic efficacy in hippocampal slices (or lack thereof) are frequently used to describe the neurologic phenotype of cognitively-impaired animals and/or to evaluate the mechanism of action of nootropic compounds. This article outlines the procedures we use for preparing hippocampal slices from rats and transgenic mice for the study of synaptic alterations associated with brain aging and Alzheimer's disease (AD)1-3. Use of aged rats and AD model mice can present a unique set of challenges to researchers accustomed to using younger rats and/or mice in their research. Aged rats have thicker skulls and tougher connective tissue than younger rats and mice, which can delay brain extraction and/or dissection and consequently negate or exaggerate real age-differences in synaptic function and plasticity. Aging and amyloid pathology may also exacerbate hippocampal damage sustained during the dissection procedure, again complicating any inferences drawn from physiologic assessment. Here, we discuss the steps taken during the dissection procedure to minimize these problems. Examples of synaptic responses acquired in "healthy" and "unhealthy" slices from rats and mice are provided, as well as representative synaptic plasticity experiments. The possible impact of other methodological factors on synaptic function in these animal models (e.g. recording solution components, stimulation parameters) are also discussed. While the focus of this article is on the use of aged rats and transgenic mice, novices to slice physiology should find enough detail here to get started on their own studies, using a variety of rodent models.

This article outlines procedures for preparing hippocampal slices from rats and transgenic mice for the study of synaptic alterations associated with brain aging and age-related neurodegenerative diseases, such as Alzheimer&#x2019;s disease.

The rodent hippocampal slice preparation is perhaps the most broadly used tool for investigating mammalian synaptic function and plasticity. The ...

Isolation of CA1 Nuclear Enriched Fractions from Hippocampal Slices to Study Activity-dependent Nuclear Import of Synapto-nuclear Messenger Proteins

Studying activity dependent protein expression, subcellular translocation, or phosphorylation is essential to understand the underlying cellular mechanisms of synaptic plasticity. Long-term potentiation (LTP) and long-term depression (LTD) induced in acute hippocampal slices are widely accepted as cellular models of learning and memory. There are numerous studies that use live cell imaging or immunohistochemistry approaches to visualize activity dependent protein dynamics. However these methods rely on the suitability of antibodies for immunocytochemistry or overexpression of fluorescence-tagged proteins in single neurons. Immunoblotting of proteins is an alternative method providing independent confirmation of the findings.&#160;The first limiting factor in preparation of subcellular fractions from individual tetanized hippocampal slices is the low amount of material. Second, the handling procedure is crucial because even very short and minor manipulations of living slices might induce activation of certain signaling cascades. Here we describe an optimized workflow in order to obtain sufficient quantity of nuclear enriched fraction of sufficient purity from the CA1 region of acute hippocampal slices from rat brain. As a representative example we show that the ERK1/2 phosphorylated form of the synapto-nuclear protein messenger Jacob actively translocates to the nucleus upon induction of LTP and can be detected in a nuclear enriched fraction from CA1 neurons.

We provide a detailed protocol for induction of long-term potentiation in the CA1 region of the hippocampus and the subsequent isolation of nuclear enriched fractions from the tetanized area of the slice. This approach can be used to determine activity dependent nuclear protein import in cellular models of learning and memory.

Studying activity dependent protein expression, subcellular translocation, or phosphorylation is essential to understand the underlying cellular ...

Brain Source Imaging in Preclinical Rat Models of Focal Epilepsy using High-Resolution EEG Recordings

Electroencephalogram (EEG) has been traditionally used to determine which brain regions are the most likely candidates for resection in patients with focal epilepsy. This methodology relies on the assumption that seizures originate from the same regions of the brain from which interictal epileptiform discharges (IEDs) emerge. Preclinical models are very useful to find correlates between IED locations and the actual regions underlying seizure initiation in focal epilepsy. Rats have been commonly used in preclinical studies of epilepsy1; hence, there exist a large variety of models for focal epilepsy in this particular species. However, it is challenging to record multichannel EEG and to perform brain source imaging in such a small animal. To overcome this issue, we combine a patented-technology to obtain 32-channel EEG recordings from rodents2 and an MRI probabilistic atlas for brain anatomical structures in Wistar rats to perform brain source imaging. In this video, we introduce the procedures to acquire multichannel EEG from Wistar rats with focal cortical dysplasia, and describe the steps both to define the volume conductor model from the MRI atlas and to uniquely determine the IEDs. Finally, we validate the whole methodology by obtaining brain source images of IEDs and compare them with those obtained at different time frames during the seizure onset.

This video introduces the preparation, recording, and source analysis procedures of high-resolution EEG on sedated rats with a particular preclinical model of focal epilepsy under noninvasive conditions.

Electroencephalogram (EEG) has been traditionally used to determine which brain regions are the most likely candidates for resection in patients with ...

Medicine

Non-restraining EEG Radiotelemetry: Epidural and Deep Intracerebral Stereotaxic EEG Electrode Placement

Implantable EEG radiotelemetry is of central relevance in the neurological characterization of transgenic mouse models of neuropsychiatric and neurodegenerative diseases as well as epilepsies. This powerful technique does not only provide valuable insights into the underlying pathophysiological mechanisms, i.e., the etiopathogenesis of CNS related diseases, it also facilitates the development of new translational, i.e., therapeutic approaches. Whereas competing techniques that make use of recorder systems used in jackets or tethered systems suffer from their unphysiological restraining to semi-restraining character, radiotelemetric EEG recordings overcome these disadvantages. Technically, implantable EEG radiotelemetry allows for precise and highly sensitive measurement of epidural and deep, intracerebral EEGs under various physiological and pathophysiological conditions. First, we present a detailed protocol of a straight forward, successful, quick and efficient technique for epidural (surface) EEG recordings resulting in high-quality electrocorticograms. Second, we demonstrate how to implant deep, intracerebral EEG electrodes, e.g., in the hippocampus (electrohippocampogram). For both approaches, a computerized 3D stereotaxic electrode implantation system is used. The radiofrequency transmitter itself is implanted into a subcutaneous pouch in both mice and rats. Special attention also has to be paid to pre-, peri- and postoperative treatment of the experimental animals. Preoperative preparation of mice and rats, suitable anesthesia as well as postoperative treatment and pain management are described in detail.

Non-restraining EEG radiotelemetry is a valuable methodological approach to record in vivo long-term electroencephalograms from freely moving rodents. This detailed protocol describes stereotaxic epidural and deep intracerebral electrode placement in different brain regions in order to obtain reliable recordings of CNS rhythmicity and CNS related behavioral stages.

Implantable EEG radiotelemetry is of central relevance in the neurological characterization of transgenic mouse models of neuropsychiatric and ...

Chronic Transcranial Electrical Stimulation and Intracortical Recording in Rats

Transcranial electrical stimulation (TES) is a powerful and relatively simple approach to diffusely influence brain activity either randomly or in a closed-loop event-triggered manner. Although many studies are focusing on the possible benefits and side-effects of TES in healthy and pathologic brains, there are still many fundamental open questions regarding the mechanism of action of the stimulation. Therefore, there is a clear need for a robust and reproducible method to test the acute and the chronic effects of TES in rodents. TES can be combined with regular behavioral, electrophysiological, and imaging techniques to investigate neuronal networks in vivo. The implantation of transcranial stimulation electrodes does not impose extra constraints on the experimental design while it offers a versatile, flexible tool to manipulate brain activity. Here we provide a detailed, step-by-step protocol to fabricate and implant transcranial stimulation electrodes to influence brain activity in a temporally constrained manner for months.

This detailed protocol describes transcranial stimulation electrode placement on the temporal bone in order to investigate the short- and long-term effects of transcranial electrical stimulation in freely moving rats.

Transcranial electrical stimulation (TES) is a powerful and relatively simple approach to diffusely influence brain activity either randomly or in a ...

Recording and Modulation of Epileptiform Activity in Rodent Brain Slices Coupled to Microelectrode Arrays

Temporal lobe epilepsy (TLE) is the most common partial complex epileptic syndrome and the least responsive to medications. Deep brain stimulation (DBS) is a promising approach when pharmacological treatment fails or neurosurgery is not recommended. Acute brain slices coupled to microelectrode arrays (MEAs) represent a valuable tool to study neuronal network interactions and their modulation by electrical stimulation. As compared to conventional extracellular recording techniques, they provide the added advantages of a greater number of observation points and a known inter-electrode distance, which allow studying the propagation path and speed of electrophysiological signals. However, tissue oxygenation may be greatly impaired during MEA recording, requiring a high perfusion rate, which comes at the cost of decreased signal-to-noise ratio and higher oscillations in the experimental temperature. Electrical stimulation further stresses the brain tissue, making it difficult to pursue prolonged recording/stimulation epochs. Moreover, electrical modulation of brain slice activity needs to target specific structures/pathways within the brain slice, requiring that electrode mapping be easily and quickly performed live during the experiment. Here, we illustrate how to perform the recording and electrical modulation of 4-aminopyridine (4AP)-induced epileptiform activity in rodent brain slices using planar MEAs. We show that the brain tissue obtained from mice outperforms rat brain tissue and is thus better suited for MEA experiments. This protocol guarantees the generation and maintenance of a stable epileptiform pattern that faithfully reproduces the electrophysiological features observed with conventional field potential recording, persists for several hours, and outlasts sustained electrical stimulation for prolonged epochs. Tissue viability throughout the experiment is achieved thanks to the use of a small-volume custom recording chamber allowing for laminar flow and quick solution exchange even at low (1 mL/min) perfusion rates. Quick MEA mapping for real-time monitoring and selection of stimulating electrodes is performed by a custom graphic user interface (GUI).

We illustrate how to perform recording and electrical modulation of 4-aminopyridine-induced epileptiform activity in rodent brain slices using microelectrode arrays. A custom recording chamber maintains tissue viability throughout prolonged experimental sessions. Live electrode mapping and selection of stimulating pairs are performed by a custom graphical user interface.

Temporal lobe epilepsy (TLE) is the most common partial complex epileptic syndrome and the least responsive to medications. Deep brain stimulation (DBS) ...

Microdialysis of Excitatory Amino Acids During EEG Recordings in Freely Moving Rats

Microdialysis is a well-established neuroscience technique that correlates the changes of neurologically active substances diffusing into the brain interstitial space with the behavior and/or with the specific outcome of a pathology (e.g., seizures for epilepsy). When studying epilepsy, the microdialysis technique is often combined with short-term or even long-term video-electroencephalography (EEG) monitoring to assess spontaneous seizure frequency, severity, progression and clustering. The combined microdialysis-EEG is based on the use of several methods and instruments. Here, we performed in vivo microdialysis and continuous video-EEG recording to monitor glutamate and aspartate outflow over time, in different phases of the natural history of epilepsy in a rat model. This combined approach allows the pairing of changes in the neurotransmitter release with specific stages of the disease development and progression. The amino acid concentration in the dialysate was determined by liquid chromatography. Here, we describe the methods and outline the principal precautionary measures one should take during in vivo microdialysis-EEG, with particular attention to the stereotaxic surgery, basal and high potassium stimulation during microdialysis, depth electrode EEG recording and high-performance liquid chromatography analysis of aspartate and glutamate in the dialysate. This approach may be adapted to test a variety of drug or disease induced changes of the physiological concentrations of aspartate and glutamate in the brain. Depending on the availability of an appropriate analytical assay, it may be further used to test different soluble molecules when employing EEG recording at the same time.

Here, we describe a method for in vivo microdialysis to analyze aspartate and glutamate release in the ventral hippocampus of epileptic and non-epileptic rats, in combination with EEG recordings. Extracellular concentrations of aspartate and glutamate may be correlated with the different phases of the disease.

Microdialysis is a well-established neuroscience technique that correlates the changes of neurologically active substances diffusing into the brain ...

Preparation of Acute Human Hippocampal Slices for Electrophysiological Recordings

Epilepsy affects about 1% of the world population and leads to a severe decrease in quality of life due to ongoing seizures as well as high risk for sudden death. Despite an abundance of available treatment options, about 30% of patients are drug-resistant. Several novel therapeutics have been developed using animal models, though the rate of drug-resistant patients remains unaltered. One of probable reasons is the lack of translation between rodent models and humans, such as a weak representation of human pharmacoresistance in animal models. Resected human brain tissue as a preclinical evaluation tool has the advantage to bridge this translational gap. Described here is a method for high quality preparation of human hippocampal brain slices and subsequent stable induction of epileptiform activity. The protocol describes the induction of burst activity during application of 8 mM KCl and 4-aminopyridin. This activity is sensitive to established AED lacosamide or novel antiepileptic candidates, such as dimethylethanolamine (DMEA). In addition, the method describes induction of seizure-like events in CA1 of human hippocampal brain slices by reduction of extracellular Mg2+ and application of bicuculline, a GABAA receptor blocker. The experimental set-up can be used to screen potential antiepileptic substances for their effects on epileptiform activity. Furthermore, mechanisms of action postulated for specific compounds can be validated using this approach in human tissue (e.g., using patch-clamp recordings). To conclude, investigation of vital human brain tissue ex vivo (here, resected hippocampus from patients suffering from temporal lobe epilepsy) will improve the current knowledge of physiological and pathological mechanisms in the human brain.

The presented protocol describes the transport and preparation of resected human hippocampal tissue with the ultimate goal to use vital brain slices as a preclinical evaluation tool for potential antiepileptic substances.

Epilepsy affects about 1% of the world population and leads to a severe decrease in quality of life due to ongoing seizures as well as high risk for ...

Assessment of Excitatory Neurotransmitter Levels in Chronic Epilepsy-Induced Rats

<a href='https://app-jove-com.remotexs.ntu.edu.sg/v/58455/microdialysis-excitatory-amino-acids-during-eeg-recordings-freely'>Source: Soukupov&#225;, M., et al. Microdialysis of Excitatory Amino Acids During EEG Recordings in Freely Moving Rats. J. Vis. Exp. (2018)</a>This video demonstrates the assessment of extracellular excitatory neurotransmitter levels in rats with chronic epilepsy induction. After implanting a microdialysis probe into the brain and confirming the absence of seizures using electroencephalography (EEG), extracellular fluid is collected to evaluate elevated neurotransmitter levels in epileptic rats. A high-potassium solution is then infused to sustain neuronal excitability and trigger an increased release of neurotransmitters, with samples collected to assess the potassium-induced peak in excitatory neurotransmitters.

Source: Soukupov&#225;, M., et al. Microdialysis of Excitatory Amino Acids During EEG Recordings in Freely Moving Rats. J. Vis. Exp. (2018)This video ...

JoVE Encyclopedia of Experiments

Neuropathology

Epilepsy and Seizure Disorders

Electroencephalographic Recording of Epileptic Seizures in Epilepsy-Induced Rats

Source: Soukupov&#225;, M., et al. <a href="https://app-jove-com.remotexs.ntu.edu.sg/v/58455">Microdialysis of Excitatory Amino Acids During EEG Recordings in Freely Moving Rats.</a> J. Vis. Exp. (2018)
This video demonstrates electroencephalographic (EEG) recording of epileptic seizures in epilepsy-induced rats. A rat with electrodes implanted in the ventral hippocampus is connected to the EEG recording system and placed in a plexiglass chamber. The rat is allowed to move freely while the brain activity is recorded to monitor the occurrence of seizures.

All procedures involving animal models have been reviewed by the local institutional animal care committee and the JoVE veterinary review board.
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Electroconvulsive Seizures in Rats and Fractionation of Their Hippocampi to Examine Seizure-induced Changes in Postsynaptic Density Proteins

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