We are grateful to Austin Ferro and Juao-Guilherme Rosa in the Cvetanovic lab for their help in troubleshooting dissections and in RNA extraction and RTqPCR. This research is funded by M. Cvetanovic, R01 NS197387; HHS | National Institutes of Health (NIH).

1. Setup
<ol>
	<li>Gather necessary equipment including decapitation scissors, blunt forceps, dissection scissors, vascular scissors, microspatula, sagittal mouse brain matrix, razor blades, 200 &#181;L&#160;pipet tips, glass petri dish, glass slide, and ice bucket. Lay out all equipment on an absorbent pad.</li>
	<li>Place petri dish, glass plate, and brain matrix on ice.</li>
	<li>Using a razor blade at a perpendicular angle, trim about 5 mm off the tip of one 200 &#181;L&#160;pipet tip. This makes the size of the opening at the end of the tip about 1 mm wide. This should be sufficient to punch out the DCN. But this can also be adjusted as needed depending on the dissection. Have many tips ready for easy replacement and adjustment.</li>
	<li>Label 1.5 mL microfuge tubes with animal identification and cerebellar region (four tubes per animal).</li>
	<li>Fill cryosafe container with liquid nitrogen to flash freeze tissue after extraction.</li>
</ol>
2. Brain extraction and dissection
All experiments were conducted in accordance with the guidelines of the Animal Care Committees of the University of Minnesota.
<ol>
	<li>Euthanize the mouse using 5% CO2 exposure. Once breathing has ceased, perform cervical dislocation. Decapitate the mouse with the decapitation scissors and discard the carcass in the appropriate receptacle.</li>
	<li>Make an incision with a razor blade along the medial sagittal line of the head starting at the nose and continuing all the way back. Separate the skin, parting to either side of the midline. Use the razor blade to cut away the muscle on each side, cutting down past the ear canals.</li>
	<li>Using dissecting scissors, trim any spinal cord regions, up to where the brain stem meets the cerebellum, careful to not damage the cerebellum.</li>
	<li>Insert one of the vascular scissor blades into the space between the brainstem and vertebral column and cut toward the ear canal, lifting up on the scissors to cleanly cut the bone but limit damage to the tissue.</li>
	<li>Continue to cut along the edge of the skull up toward the olfactory bulbs, continuing to lift up while cutting to limit damage to the brain tissue.</li>
	<li>Using the blunt forceps, gently peel off the back of the skull uncovering the posterior region of the brain and cerebellum.</li>
	<li>Using the blunt forceps along the edge of the skull that was just cut, peel the rest of the skull up and over the brain. This step should remove the majority of the skull cap, revealing the brain.</li>
	<li>Trim the rest of the skull with the vascular scissors and blunt forceps, clearing most of the skull from the top of the brain.</li>
	<li>Using the microspatula, lift the brain slightly and scoop under and slide up to remove the olfactory bulbs from the remaining skull and disconnect optic tract fibers. Brain should come free easily at this point.</li>
	<li>Place the brain into the petri dish sitting on ice and remove any remaining skull or other debris.</li>
	<li>Using the microspatula, gently place the brain into the brain matrix with dorsal side up. Take time to make sure it is set level in the matrix, especially that the midline falls center in the matrix. This matrix is designed for adult mouse brain tissue, tissue from younger or diseased animals may rest lower in the matrix but it should still be possible to achieve reproducible results across samples.</li>
	<li>Place one razor blade along the sagittal midline, making sure that the blade pushes all the way to the bottom of the matrix (Figure 1B).</li>
	<li>Place another razor blade 1 mm to the side of the first blade (Figure 1B). Place two more blades 1 mm apart from each other. The end result should be three blades placed on one side of the brain, all 1mm apart. Do the same to the other side. In total, 7 blades will be placed 1mm apart (Figure 1C).</li>
	<li>Carefully, grab the front and back ends of the razor blades and lift straight up out of the matrix. The tissue on the outside of the razor blades can be discarded.</li>
	<li>Slowly, separate one razor blade at a time from the others, being careful not to damage the tissue sections.</li>
	<li>Carefully slide the tissue section off of the razor blade and onto the glass slide with the microspatula. In total there will be six sagittal brain sections (Figure 1D).</li>
	<li>The 4 most lateral sections will have DCN visible (Purple box, Figure 1D). To isolate the DCN, hold the trimmed 200 &#181;L&#160;pipet tip perpendicularly over the DCN and push down through the tissue firmly, rocking in all directions to fully dissect the DCN from surrounding tissue. Lift straight back up to cleanly remove the DCN, and visually confirm the presence of the tissue in the tip.</li>
	<li>Place one finger at the top of the tip and push down, causing the tissue to bulge out. Place the tip into correctly labeled microfuge tube and ensure that tissue punch is placed in the bottom of the tube. Repeat 2.17 for the remaining three sections, placing the DCN punches in the same tube. Place the tube into liquid nitrogen to flash freeze. Representation of size of each punch in Figure 1E.</li>
	<li>Sections that had DCN extracted qualify as cerebellar hemisphere. Push away the rest of the brain tissue around the cerebellum in these sections. Use blunt forceps and gently pick up these hemisphere cerebellar cortex sections and place into respective microfuge tube. Flash freeze.</li>
	<li>For the last two vermal sections (light blue box, Figure1D), push away surrounding brain tissue leaving only the cerebellum. Using a razor blade, make a cut separating the anterior lobules from the posterior lobules. Cut should be just after the formation of lobule 6 and should not include lobule 10 (Figure 1F).</li>
	<li>Using blunt forceps, carefully place the anterior cerebellar cortex sections and posterior cerebellar cortex sections into their respective microfuge tubes and flash freeze by leaving the tubes in liquid nitrogen for 5 minutes. From here move forward to RNA extraction, or may &#160;store the tubes at -80 &#730;C.</li>
</ol>
3. RNA extraction 
NOTE: This protocol is modified from the Cold Spring Harbor Protocol for RNA Extraction with TRIzol20. TRIzol solubilizes biological material, making it possible to extract RNA.
<ol>
	<li>Place the microfuge tubes in ice to keep the tissue from thawing too quickly, apply 150 &#181;L&#160;of cold TRIzol in the microfuge tube. Homogenize with a sterilized pestle. Once tissue is homogenized, pipet the solution up and down to ensure there is no remaining tissue intact. Further break up any small tissue pieces by pulling it up into an insulin syringe a few times.</li>
	<li>Add another 350 &#181;L&#160;of TRIzol and pipet up and down to mix thoroughly. Let sit at room temp for 5 minutes.</li>
	<li>Add 150 &#181;L&#160;of chloroform to the tube and shake vigorously and then let rest for 2-3 minutes. The chloroform separates the homogenized tissue solution into phases (RNA, DNA, and protein).</li>
	<li>Centrifuge at 12,000 x g, at 15&#730;C, for 10 minutes. Ensure that all tubes are at the same orientation.</li>
	<li>Carefully remove the tubes and set the temperature of the centrifuge to 4&#730;C. Remove only the clear aqueous phase into a new tube (this is the RNA), careful not to disrupt the opaque interphase (the DNA). &#160;The lowest phase will be red and contains protein. Remaining solution in the tubes can be saved or discarded.</li>
	<li>Add 100% isopropyl alcohol at a 1:2 ratio (if removed 200 ul of aqueous phase, add 100 &#181;L&#160;of isopropyl alcohol). Mix thoroughly by pipetting up and down. Let rest at room temperature for 10 minutes. The isopropyl alcohol precipitates the RNA out of solution.</li>
	<li>Centrifuge at 12,000 x g, at 4&#730;C, for 10 minutes. Be sure to place all the tubes at the same orientation to make it easier to visualize the pellet. The resulting pellet will be the extracted RNA.</li>
	<li>Carefully remove the tubes, remove the supernatant with a pipet being careful not to disrupt the pellet. The pellet is somewhat gel-like and will be difficult to see, but should be able to estimate where it is based on the orientation of the tubes in the centrifuge.</li>
	<li>After removing all of the supernatant, add 500 &#181;L&#160;of 75% ethanol, vortex briefly, and centrifuge at 7500 x g, at 4&#730;C, for 5 minutes. The ethanol further washes the pellet.</li>
	<li>Remove the supernatant carefully, without disrupting the pellet. Leave caps open to dry the sample. This usually takes 5-10 minutes but can vary depending on how much ethanol was left on the pellet. Do not over dry.</li>
	<li>Once dry, resuspend the pellet in DNase free water. Add 20 &#181;L&#160;to samples for DCN, and 30 &#181;L&#160;for all others.</li>
	<li>Once resuspended, samples can be stored at -80 &#730;C or proceed to further testing.</li>
</ol>
4. Real Time quantitative Polymerase Chain Reaction (RTqPCR)
<ol>
	<li>Before this step it will be necessary to DNase treat the RNA to remove any genomic DNA, and generate cDNA utilizing iScript from BioRad. Be sure to normalize the concentration of RNA before making the cDNA. In addition, it is important to optimize primers for qPCR. Follow the methods described here to complete this step21. Brief description of the qPCR below.</li>
	<li>Primers are all purchased from IDT. Forward and reverse sequences are both in the same sample tube, and stored at 20x concentration. 
	Rps18 (control gene): 
	Forward &#8211; 5&#8217;-CCTGAGAAGTTCCAGCACAT-3&#8217; 
	Reverse &#8211; 5&#8217;-ACACCACATGAGCATATCTCC-3&#39; 
	Parvalbumin (Calcium binding protein, inhibitory cells): 
	Forward &#8211; &#8216;5-ATGAGGTGAAGAAGGTGTTCC-3&#8217; 
	Reverse &#8211; &#8216;5-AGCGTCTTTGTTTCTTTAGCAG-3&#8217; 
	Kcng4 (Potassium channel subunit): 
	Forward &#8211; 5&#8217;-CTGTCTTTTCCTGGTCAGTGA-3&#8217; 
	Reverse &#8211; 5&#8217;-GCATTGCCTCAGACTGTCAG-3&#8217; 
	Aldolase C (Zebrin II, differentially expressed across the cerebellar cortex): 
	Forward &#8211; 5&#8217;-AGAGGACAAAGGGATAATGCTG-3&#8217; 
	Reverse &#8211; 5&#8217;-TCAGTAGGCATGGTTGGC-3&#8217;</li>
	<li>qPCR conditions were as follows. Pre-incubation period, 5 minutes, at 95&#730;C. Amplification period, 50 cycles: 10 minutes at 95&#730;C, 10 minutes at 62&#730;C, and 10 minutes at 72&#730;C. Melting curve period, 5 seconds at 95&#730;C, one minute at 65&#730;C, and set ramp rate to .07&#730;C/second until target temp of 97&#730;C. Then cooling period for 10 minutes to 40&#730;C. &#160;All qPCR reactions were performed in triplicate and gene expression was analyzed using 2- &#916;&#916;Ct with Rps18 as a loading control to normalize gene expression. Bulk cerebellar extract was used as a reference.</li>
</ol>

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The authors have nothing to disclose.

The method described here makes it possible to assess the underlying gene expression and molecular mechanisms within four distinct cerebellar regions &#8211; the deep cerebellar nuclei (DCN), the anterior cerebellar cortex of the vermis (CCaV), the posterior cerebellar cortex of the vermis (CCpV), and the cerebellar cortex of the hemispheres (CCH). The ability to assess these regions separately will expand our knowledge of the heterogeneity of specific cerebellar regions and possibly shed light on their contribution to v...

The cerebellum contains over half of the neurons in the brain and has historically been referred to as a motor control and balance center in the brain1. More recently, studies have demonstrated that the cerebellum plays a key role in various other functions including cognition, reward processing, and affect2,3,4,5.
The cerebellum has well-described anatomy: the cortex region is composed of granule, Purkinje, and molecular layers. Granule cells form the granule cell layer and send input via parallel fibers to the Purkinje cell dendrites of the molecular layer which also receive input from climbing fibers that originated in the inferior olive. Purkinje cells send inhibitory projections to cells in the deep cerebellar nuclei (DCN), which serves as the main output from the cerebellum. The output of this cerebellar circuit is further modulated by the activity of the inhibitory interneurons in the cerebellar cortex, including Golgi, stellate, and basket cells4. This cerebellar functional unit is distributed throughout all the lobules of the cerebellar cortex. Despite this relatively uniform circuitry across &#160;the cerebellum, evidence from human neuroimaging literature and patient studies indicates functional heterogeneity of the cerebellum6,7.
The cerebellar cortex can be divided into two main regions: the midline-defined vermis, and the lateral hemispheres. The vermis can be further divided into anterior and posterior lobules. These distinct regions of the cerebellum have been implicated in contributing to different behaviors. Task-evoked or task-free activity patterns implicated that anterior regions of the vermis contribute more to motor function while posterior vermis contributes more to cognition6,7. The vermis is also linked with affect and emotions, while cerebellar hemispheres contribute to executive, visual-spatial, language, and other mnemonic functions8. In addition, anatomical studies provided evidence that functionally distinct cerebellar regions are connected with different cortical regions9. Lesion-symptom mapping revealed that patients with strokes affecting the anterior lobules (extending into lobule VI) had poorer performance on fine motor tasks, while patients with damage to posterior lobe regions and hemispheres exhibited cognitive deficits in the absence of cerebellar motor syndrome10. Finally, regional cerebellar pathology in disease indicates that functionally distinct cerebellar regions are also differently susceptible to disease11,12.
While much less explored, preliminary evidence demonstrates distinct gene expression signatures across cerebellar cortical regions. Purkinje cell expression of Zebrin II shows region specific patterning in the vermis such that there are more Zebrin II positive cells in the posterior lobules and fewer in the anterior lobules13. This also correlates with regionally distinct physiological function as Zebrin II negative Purkinje cells display higher frequency of tonic firing than Purkinje cells that are Zebrin II positive14.
In addition to the cerebellar cortex, the cerebellum includes the deep cerebellar nuclei (DCN) which serve as the primary output for the cerebellum. The nuclei are made up of the medial (MN), interposed (IN), and lateral nuclei (LN). Functional imaging and patient studies have demonstrated that the DCN also participate in various behaviors15, but very few studies examine gene expression change in DCN.
Advances in molecular techniques have made it possible to assess regional gene expression in the brain and have uncovered heterogeneity across and within different brain regions in both physiological and disease states16. Such studies implicate that the cerebellum is different from other brain regions. For example, the ratio of neurons to glial cells is inverted in the cerebellum&#160; compared to other brain regions1. Even in normal physiological conditions, the expression of proinflammatory genes is upregulated in the cerebellum compared to the other brain regions17. Molecular techniques have also been very useful in identifying the pathways that contribute to the pathogenesis of cerebellar diseases. For instance, RNA sequencing of the whole cerebellar extracts identified genes altered in a Purkinje cell specific transgenic mouse model of spinocerebellar ataxia type 1 (SCA1) as compared to their wild type controls. Such evidence has revealed key molecular pathways underlying pathogenesis in cerebellar Purkinje cells and has helped identify potential therapeutic targets18. However, recent studies suggest that there are differences in the vulnerability to diseases across the cerebellar regions11,12,19. This could indicate that there are key changes occurring in distinct cerebellar regions, which may be masked or undetected with whole cerebellar extracts. Thus, there is a need to develop techniques which allow researchers to examine molecular profiles in different cerebellar regions.
The technique proposed here describes a reproducible method to dissect four distinct regions of the mouse cerebellum in order to isolate RNA from those regions and explore regional differences in gene expression. The schematic of the mouse cerebellum in Figure 1A highlights the vermis in blue, and hemispheres in yellow. Specifically, this technique makes it possible to isolate four regions:&#160; deep cerebellar nuclei (DCN) (red-dotted boxes in Figure 1A), the cerebellar cortex of anterior vermis (CCaV) (dark blue in Figure 1A), the cerebellar cortex of the posterior vermis (CCpV) (light blue in Figure 1A), and the cerebellar cortex of the hemispheres (CCH) (yellow in Figure 1A). By assessing gene expression of these regions separately, it will be possible to investigate molecular mechanisms underlying discrete functions of these different regions as well as potential differences in their vulnerability in disease.

<table><tbody><tr><td>1.5 Microcentrifuge tubes</td><td>ThermoScietific</td><td>3456</td><td></td></tr><tr><td>100% Isopropyl Alcohol</td><td>VWR Life sciences</td><td>1106C361</td><td></td></tr><tr><td>200 ul Pipet tips</td><td>GeneMate</td><td>P-1237-200</td><td></td></tr><tr><td>Adult Mouse Brain Matrix Sagittal</td><td>Kent Scientific Corporation</td><td>RBMA-200S</td><td></td></tr><tr><td>Blunt forceps</td><td></td><td></td><td></td></tr><tr><td>Chloroform</td><td>Macron</td><td>220905</td><td></td></tr><tr><td>Decapitation Scissors</td><td></td><td></td><td></td></tr><tr><td>Dissecting Scissors</td><td></td><td></td><td></td></tr><tr><td>Ethyl Alcohol</td><td>Pharmco</td><td>111000200</td><td></td></tr><tr><td>Glass Slide (for electrophoresis)</td><td>BIORAD</td><td></td><td></td></tr><tr><td>Homogenizer</td><td>Kimble</td><td>6HAZ6</td><td></td></tr><tr><td>Ice Bucket</td><td></td><td></td><td></td></tr><tr><td>Insulin Syringe (.5ml)</td><td>BD</td><td>329461</td><td></td></tr><tr><td>iScript Adv cDNA kit for RT-qPCR</td><td>BIORAD</td><td>1725037</td><td></td></tr><tr><td>Micro Spatula</td><td></td><td></td><td></td></tr><tr><td>Needle Nose forceps</td><td></td><td></td><td></td></tr><tr><td>Petri Dish</td><td>Pyrex</td><td></td><td></td></tr><tr><td>Primetime Primer for Aldolase C</td><td>IDT</td><td>Mm.PT.58&gt;43415246</td><td></td></tr><tr><td>Primetime Primer for Kcng4</td><td>IDT</td><td>Mm.PT.56a.9448518</td><td></td></tr><tr><td>Primetime Primer for Parvalbumin</td><td>IDT</td><td>Mm.PT.58.7596729</td><td></td></tr><tr><td>Primetime Primer Rps18&amp;nbsp;</td><td>IDT</td><td>Mm.PT.58.12109666</td><td></td></tr><tr><td>Single Edge Rzor Blades</td><td>Personna GEM</td><td></td><td></td></tr><tr><td>Sterile, sigle-use pestles</td><td>FisherScientific</td><td>12141364</td><td></td></tr><tr><td>TRIzol Reagent</td><td>Ambion by Life technologies</td><td>15596018</td><td></td></tr><tr><td>Vascular Scissors</td><td></td><td></td><td></td></tr></tbody></table>

cerebellar regional dissection for molecular analysis

Cerebellum plays an important role in several key functions including control of movement, balance, cognition, reward, and affect. Imaging studies indicate that distinct cerebellar regions contribute to these different functions. Molecular studies examining regional cerebellar differences are lagging as they are mostly done on whole cerebellar extracts thereby masking any distinctions across specific cerebellar regions. Here we describe a technique to reproducibly and quickly dissect four different cerebellar regions: the deep cerebellar nuclei (DCN), anterior and posterior vermal cerebellar cortex, and the cerebellar cortex of the hemispheres. Dissecting out these distinct regions allows for the exploration of molecular mechanisms that may underlie their unique contributions to balance, movement, affect and cognition. This technique may also be used to explore differences in pathological susceptibility of these specific regions across various mouse disease models.

For these experiments, four eleven-week-old female wild type C57/Black6 mice were used. One mouse was used to conduct a full cerebellar dissection which is referred to as &#39;bulk cerebellum&#39; and allowed for the comparison of RNA levels in dissected regions to a full dissection. The other three mice were used to conduct the cerebellar dissection described in this protocol. Using three mice makes it possible to ensure that the trends detected in the levels of RNA are reproducible acro...

Watch this Scientific Journal Video about Cerebellar Regional Dissection for Molecular Analysis at JoVE.com

Cerebellar Regional Dissection for Molecular Analysis

Different cerebellar regions have been implicated to play a role in distinct behavioral outputs, yet the underlying molecular mechanisms remain unknown. This work describes a method to reproducibly and quickly dissect cerebellar cortex of the hemispheres, anterior and posterior regions of the vermis, and the deep cerebellar nuclei in order to probe for molecular differences by isolating RNA and testing for differences in gene expression.&#160;

Cerebellum plays an important role in several key functions including control of movement, balance, cognition, reward, and affect. Imaging studies ...

cerebellar-regional-dissection-for-molecular-analysis

Research

JoVE Journal

Neuroscience

4.4K Views.  University of Minnesota. Verschillende cerebellaire regio's zijn betrokken om een rol te spelen in verschillende gedragsoutputs, maar de onderliggende moleculaire mechanismen blijven onbekend. Dit werk beschrijft een methode om de cerebellaire cortex van de hemisferen, voorste en achterste gebieden van de vermis en de diepe cerebellaire kernen reproduceerbaar en snel te ontleden om moleculaire verschillen te onderzoeken door RNA te isoleren en te testen op verschillen in genexpressie.

Video: Cerebellar Regional Dissection for Molecular Analysis

Wholemount Immunohistochemistry for Revealing Complex Brain Topography

The repeated and well-understood cellular architecture of the cerebellum make it an ideal model system for exploring brain topography. Underlying its relatively uniform cytoarchitecture is a complex array of parasagittal domains of gene and protein expression. The molecular compartmentalization of the cerebellum is mirrored by the anatomical and functional organization of afferent fibers. To fully appreciate the complexity of cerebellar organization we previously refined a wholemount staining approach for high throughput analysis of patterning defects in the mouse cerebellum. This protocol describes in detail the reagents, tools, and practical steps that are useful to successfully reveal protein expression patterns in the adult mouse cerebellum by using wholemount immunostaining. The steps highlighted here demonstrate the utility of this method using the expression of zebrinII/aldolaseC as an example of how the fine topography of the brain can be revealed in its native three-dimensional conformation. Also described are adaptations to the protocol that allow for the visualization of protein expression in afferent projections and large cerebella for comparative studies of molecular topography. To illustrate these applications, data from afferent staining of the rat cerebellum are included.

Neural circuits are topographically organized into functional compartments with specific molecular profiles. Here, we provide the practical and technical steps for revealing global brain topography using a versatile wholemount immunohistochemical staining approach. We demonstrate the utility of the method using the well-understood cytoarchitecture and circuitry of cerebellum.

The repeated and well-understood cellular architecture of the cerebellum make it an ideal model system for exploring brain topography. Underlying its ...

A Visual Description of the Dissection of the Cerebral Surface Vasculature and Associated Meninges and the Choroid Plexus from Rat Brain

This video presentation was created to show a method of harvesting the two most important highly vascular structures, not residing within the brain proper, that support forebrain function. They are the cerebral surface (superficial) vasculature along with associated meninges (MAV) and the choroid plexus which are necessary for cerebral blood flow and cerebrospinal fluid (CSF) homeostasis. The tissue harvested is suitable for biochemical and physiological analysis, and the MAV has been shown to be sensitive to damage produced by amphetamine and hyperthermia 1,2. As well, the major and minor cerebral vasculatures harvested in MAV are of potentially high interest when investigating concussive types of head trauma. The MAV dissected in this presentation consists of the pial and some of the arachnoid membrane (less dura) of the meninges and the major and minor cerebral surface vasculature. The choroid plexus dissected is the structure that resides in the lateral ventricles as described by Oldfield and McKinley3,4,5,6. The methods used for harvesting these two tissues also facilitate the harvesting of regional cortical tissue devoid of meninges and larger cerebral surface vasculature, and is compatible with harvesting other brain tissues such as striatum, hypothalamus, hippocampus, etc. The dissection of the two tissues takes from 5 to 10 min total. The gene expression levels for the dissected MAV and choroid plexus, as shown and described in this presentation can be found at GSE23093 (MAV) and GSE29733 (choroid plexus) at the NCBI GEO repository. This data has been, and is being, used to help further understand the functioning of the MAV and choroid plexus and how neurotoxic events such as severe hyperthermia and AMPH adversely affect their function.

This video presentation shows a method of harvesting the two most important highly vascular structures that support forebrain function. They are the cerebral surface (superficial) vasculature along with associated meninges (MAV) and the choroid plexus which are necessary for cerebral blood flow and cerebrospinal fluid (CSF) homeostasis.

This video presentation was created to show a method of harvesting the two most important highly vascular structures, not residing within the brain ...

Isolation of Distinct Cell Populations from the Developing Cerebellum by Microdissection

Microdissection is a novel technique that can isolate specific regions of a tissue and eliminate contamination from cellular sources in adjacent areas. This method was first utilized in the study of Nestin-expressing progenitors (NEPs), a newly identified population of cells in the cerebellar external germinal layer (EGL). Using microdissection in combination with fluorescent-activated cell sorting (FACS), a pure population of NEPs was collected separately from conventional granule neuron precursors in the EGL and from other contaminating Nestin-expressing cells in the cerebellum. Without microdissection, functional analyses of NEPs would not have been possible with the current methods available, such as Percoll gradient centrifugation and laser capture microdissection. This technique can also be applied for use with various tissues that contain either recognizable regions or fluorescently-labeled cells. Most importantly, a major advantage of this microdissection technique is that isolated cells are living and can be cultured for further experimentation, which is currently not possible with other described methods.

Nestin-expressing&#160;progenitors are a newly identified population of neuronal progenitors in the developing cerebellum. Using the microdissection technique presented here in combination with fluorescent-activated cell sorting, this cell population can be purified with no contamination from other cerebellar regions and can be cultured for further studies.

Microdissection is a novel technique that can isolate specific regions of a tissue and eliminate contamination from cellular sources in adjacent areas. ...

Collection of Frozen Rodent Brain Regions for Downstream Analyses

As our understanding of neurobiology has progressed, molecular analyses are often performed on small brain areas such as the medial prefrontal cortex (mPFC) or nucleus accumbens. The challenge in this work is to dissect the correct area while preserving the microenvironment to be examined. In this paper, we describe a simple, low-cost method using resources readily available in most labs. This method preserves nucleic acid and proteins by keeping the tissue frozen throughout the process. Brains are cut into 0.5&#8211;1.0 mm sections using a brain matrix and arranged on a frozen glass plate. Landmarks within each section are compared to a reference, such as the Allen Mouse Brain Atlas, and regions are dissected using a cold scalpel or biopsy punch. Tissue is then stored at -80 &#176;C until use. Through this process rat and mouse mPFC, nucleus accumbens, dorsal and ventral hippocampus and other regions have been successfully analyzed using qRT-PCR and Western assays. This method is limited to brain regions that can be identified by clear landmarks.

This procedure describes the collection of discrete frozen brain regions to obtain high-quality protein and RNA using inexpensive and commonly available tools.

As our understanding of neurobiology has progressed, molecular analyses are often performed on small brain areas such as the medial prefrontal cortex ...

Ex Vivo Myelination and Remyelination in Cerebellar Slice Cultures as a Quantitative Model for Developmental and Disease-Relevant Manipulations

Studying myelination&#160;in vitro&#160;and&#160;in vivo poses numerous challenges. The differentiation of oligodendrocyte precursor cells (OPCs)&#160;in vitro, although scalable,&#160;does not recapitulate axonal myelination. OPC-neuron cocultures and OPC-fiber cultures allow for the examination of in vitro myelination, but they lack additional cell types that are present in vivo, such as astrocytes and microglia. In vivo&#160;mouse models, however, are less amenable to chemical, environmental, and genetic manipulation and are much more labor intensive. Here, we describe&#160;an&#160;ex vivo mouse cerebellar slice culture (CSC) quantitative system that is useful for: 1) studying developmental myelination, 2) modeling demyelination and remyelination, and 3) conducting translational research. Sagittal sections of the cerebellum and hindbrain are isolated from postnatal day (P) 0&#8211;2 mice, after which they myelinate&#160;ex vivo&#160;for 12 days. During this period, slices can be manipulated in various ways, including the addition of compounds to test for an effect on developmental myelination. In addition, tissue can be fixed for electron microscopy to assess myelin ultrastructure and compaction. To model disease, CSC can be subjected to acute hypoxia to induce hypomyelination. Demyelination in these explants can also be induced by lysolecithin, which allows for the identification of factors that promote remyelination. Aside from chemical and environmental modifications, CSC can be isolated from transgenic mice and are responsive to genetic manipulation induced with Ad-Cre adenoviruses and tamoxifen. Thus, cerebellar slice cultures are a fast, reproducible, and quantifiable model for recapitulating myelination.

Presented is a protocol for an ex vivo quantitative model of demyelination and remyelination using mouse cerebellar slice cultures. This method closely recapitulates an in vivo model with its full complement of CNS cell types in intact tissue, while maintaining the chemical, genetic, and environmental amenability of an in vitro system.

Studying myelination&#160;in vitro&#160;and&#160;in vivo poses numerous challenges. The differentiation of oligodendrocyte precursor cells (OPCs)&#160;in ...

Microdissection of Mouse Brain into Functionally and Anatomically Different Regions

The brain is the command center for the mammalian nervous system and an organ with enormous structural complexity. Protected within the skull, the brain consists of an outer covering of grey matter over the hemispheres known as the cerebral cortex. Underneath this layer reside many other specialized structures that are essential for multiple phenomenon important for existence. Acquiring samples of specific gross brain regions requires quick and precise dissection steps.&#160;It is understood that at the microscopic level, many sub-regions exist and likely cross the arbitrary regional boundaries that we impose for the purpose of this dissection.
Mouse models are routinely used to study human brain functions and diseases. Changes in gene expression patterns may be confined to specific brain areas targeting a particular phenotype depending on the diseased state. Thus, it is of great importance to study regulation of transcription with respect to its well-defined structural organization. A complete understanding of the brain requires studying distinct brain regions, defining connections, and identifying key differences in the activities of each of these brain regions. A more comprehensive understanding of each of these distinct regions may pave the way for new and improved treatments in the field of neuroscience. Herein, we discuss a step-by-step methodology for dissecting the mouse brain into sixteen distinct regions. In this procedure, we have focused on male mouse C57Bl/6J (6-8 week old) brain removal and dissection into multiple regions using neuroanatomical landmarks to identify and sample discrete functionally-relevant and behaviorally-relevant&#160;brain regions. This work will help lay a strong foundation in the field of neuroscience, leading to more focused approaches in the deeper understanding of brain function.

We present a hands-on, step-by-step, rapid protocol for mouse brain removal and dissection of discrete regions from fresh brain tissue. Obtaining brain regions for molecular analysis has become routine in many neuroscience labs. These brain regions are immediately frozen to obtain high quality transcriptomic data for system level analysis.

The brain is the command center for the mammalian nervous system and an organ with enormous structural complexity. Protected within the skull, the brain ...

Cryo-section Dissection of the Adult Subependymal Zone for Accurate and Deep Quantitative Proteome Analysis

The subependymal neurogenic niche consists of a paraventricular ribbon of the lateral ventricular wall of the lateral ventricle. The subependymal zone (SEZ) is a thin and distinct region exposed to the ventricles and cerebrospinal fluid. The isolation of this niche allows the analysis of a neurogenic stem cell microenvironment. However, extraction of small tissues for proteome analysis&#160;is challenging, especially for the maintenance of considerable measurement depth and the achievement of reliable robustness. A new method termed cryo-section-dissection (CSD), combining high precision with minimal tissue perturbation, was developed to address these challenges. The method is compatible with state-of-the-art mass spectrometry (MS) methods that allow the detection of low-abundant niche regulators. This study compared the CSD and its proteome data to the method and data obtained by laser-capture-microdissection (LCM) and a standard wholemount dissection. The CSD method resulted in twice the quantification depth in less than half the preparation time compared to the LCM and simultaneously clearly outperformed the dissection precision of the wholemount dissection. Hence, CSD is a superior method for collecting the SEZ for proteome analysis.

Cryo-section-dissection allows fresh, frozen preparation of the largest neurogenic niche in the murine brain for deep quantitative proteome analysis. The method is precise, efficient, and causes minimal tissue perturbation. Therefore, it is ideally suited for studying the molecular microenvironment of this niche, as well as other organs, regions, and species.

The subependymal neurogenic niche consists of a paraventricular ribbon of the lateral ventricular wall of the lateral ventricle. The subependymal zone ...

A Standardized Pipeline for Examining Human Cerebellar Grey Matter Morphometry using Structural Magnetic Resonance Imaging

Multiple lines of research provide compelling evidence for a role of the cerebellum in a wide array of cognitive and affective functions, going far beyond its historical association with motor control. Structural and functional neuroimaging studies have further refined understanding of the functional neuroanatomy of the cerebellum beyond its anatomical divisions, highlighting the need for the examination of individual cerebellar subunits in healthy variability and neurological diseases. This paper presents a standardized pipeline for examining cerebellum grey matter morphometry that combines high-resolution, state-of-the-art approaches for optimized and automated cerebellum parcellation (Automatic Cerebellum Anatomical Parcellation using U-Net Locally Constrained Optimization; ACAPULCO) and voxel-based registration of the cerebellum (Spatially Unbiased Infra-tentorial Template; SUIT) for volumetric quantification. 
The pipeline has broad applicability to a range of neurological diseases and is fully automated, with manual intervention only required for quality control of the outputs. The pipeline is freely available, with substantial accompanying documentation, and can be run on Mac, Windows, and Linux operating systems. The pipeline is applied in a cohort of individuals with Friedreich ataxia (FRDA), and representative results, as well as recommendations on group-level inferential statistical analyses, are provided. This pipeline could facilitate reliability and reproducibility across the field, ultimately providing a powerful methodological approach for characterizing and tracking cerebellar structural changes in neurological diseases.

A standardized pipeline is presented for examining cerebellum grey matter morphometry. The pipeline combines high-resolution, state-of-the-art approaches for optimized and automated cerebellum parcellation and voxel-based registration of the cerebellum for volumetric quantification.

Multiple lines of research provide compelling evidence for a role of the cerebellum in a wide array of cognitive and affective functions, going far beyond ...

Validation of a Mouse Model to Disrupt LINC Complexes in a Cell-specific Manner

Nuclear migration and anchorage within developing and adult tissues relies heavily upon large macromolecular protein assemblies called LInkers of the Nucleoskeleton and Cytoskeleton (LINC complexes). These protein scaffolds span the nuclear envelope and connect the interior of the nucleus to components of the surrounding cytoplasmic cytoskeleton. LINC complexes consist of two evolutionary-conserved protein families, Sun proteins and Nesprins that harbor C-terminal molecular signature motifs called the SUN and KASH domains, respectively. Sun proteins are transmembrane proteins of the inner nuclear membrane whose N-terminal nucleoplasmic domain interacts with the nuclear lamina while their C-terminal SUN domains protrudes into the perinuclear space and interacts with the KASH domain of Nesprins. Canonical Nesprin isoforms have a variable sized N-terminus that projects into the cytoplasm and interacts with components of the cytoskeleton. This protocol describes the validation of a dominant-negative transgenic mouse strategy that disrupts endogenous SUN/KASH interactions in a cell-type specific manner. Our approach is based on the Cre/Lox system that bypasses many drawbacks such as perinatal lethality and cell nonautonomous phenotypes that are associated with germline models of LINC complex inactivation. For this reason, this model provides a useful tool to understand the role of LINC complexes during development and homeostasis in a wide array of tissues.

Nuclear envelope proteins play a central role in many basic biological processes and have been implicated in a variety of human diseases. This protocol describes a new Cre/Lox-based mouse model that allows for the spatiotemporal control of LINC complexes disruption.

Nuclear migration and anchorage within developing and adult tissues relies heavily upon large macromolecular protein assemblies called LInkers of the ...

Biology

Cerebellar Purkinje Cells: DNA Damage Response in Organotypic Cultures

Visualizing the DNA Damage Response in Purkinje Cells Using Cerebellar Organotypic Cultures

Cerebellar Purkinje cells (PCs) exhibit a unique interplay of high metabolic rates, specific chromatin architecture, and extensive transcriptional activity, making them particularly vulnerable to DNA damage. This necessitates an efficient DNA damage response (DDR) to prevent cerebellar degeneration, often initiated by PC dysfunction or loss. A notable example is the genome instability syndrome, ataxia-telangiectasia (A-T), marked by progressive PC depletion and cerebellar deterioration. Investigating DDR mechanisms in PCs is vital for elucidating the pathways leading to their degeneration in such disorders. However, the complexity of isolating and cultivating PCs in vitro has long hindered research efforts. Murine cerebellar organotypic (slice) cultures offer a feasible alternative, closely mimicking the in vivo tissue environment. Yet, this model is constrained to DDR indicators amenable to microscopic imaging. We have refined the organotypic culture protocol, demonstrating that fluorescent imaging of protein-bound poly(ADP-ribose) (PAR) chains, a rapid and early DDR indicator, effectively reveals DDR dynamics in PCs within these cultures, in response to genotoxic stress.

Author Spotlight: Deciphering the Role of ATM in Ataxia-Telangiectasia and the Associated Cerebellar Degeneration

Cerebellar Purkinje cells (PCs) are particularly sensitive to deficiencies in the DNA damage response. A protocol is presented for the visual evaluation of the dynamics of PC response to DNA damage, which involves staining protein-bound poly(ADP-ribose) chains within cerebellar organotypic cultures.

Cerebellar Regional Dissection for Molecular Analysis

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