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All procedures involving animal models have been reviewed by the local institutional animal care committee and the JoVE veterinary review board.
Both C57BL/6 mice and Fpr-rs3-i-Venus mice were housed in groups of both sexes at room temperature on a 12-hour light/dark cycle with food and water available ad libitum. For experiments, young adults (6-20 weeks) of either sex were used. No obvious gender-dependent differences were observed.
1. Solution Preparation
<ol>
	<li>Prepare extracellular solution S1: 4-(2-Hydroxy-ethyl)piperazine-1-ethanesulfonic acid (HEPES) buffered extracellular solution containing (in mM) 145 NaCl, 5 KCl, 1 CaCl2, 1 MgCl2, 10 HEPES; pH = 7.3 (adjusted with NaOH); osmolarity = 300 mOsm (adjusted with glucose).</li>
	<li>Prepare extracellular solution S2: Carbogen-oxygenated (95% O2, 5% CO2) extracellular solution containing (in mM) 125 NaCl, 25 NaHCO3, 5 KCl, 1 CaCl2, 1 MgSO4, 5 BES (Bis(2-hydroxyethyl)-2-aminoethanesulfonic acid); pH = 7.3; osmolarity = 300 mOsm (adjusted with glucose).</li>
	<li>Prepare 4% low-gelling temperature agarose solution (S3) for tissue embedding: 4% low-gelling temperature agarose. Dissolve 2 g low-gelling agarose in 50 ml of S1 in a 100 ml glass laboratory bottle together with a magnetic stirrer. To melt the agarose, put the bottle in a water bath (with the lid not tightly closed) at 70 &#176;C for approximately 20 min or until the solution becomes transparent while stirring. Cool down and keep melted agarose in a second water bath at 42 &#176;C until further use.</li>
	<li>Prepare intracellular solution S4: Pipette solution containing (in mM) 143 KCl, 2 KOH, 1 EGTA (ethylene glycol-bis(&#946;-aminoethyl ether)-N,N,N&#8242;,N&#8242;-tetraacetic acid), 0.3 CaCl2 (free Ca2+ = 110 nM), 10 HEPES, 2 MgATP(Magnesium Adenosine 5&#39;-triphosphate), 1 NaGTP(Guanosine 5&#8242;-triphosphate sodium salt hydrate); pH = 7.1 (adjusted with KOH); osmolarity = 290 mOsm.</li>
	<li>Modify/adjust the composition of S1, S2, and S4 according to individual experimental design (e.g., use pharmacological blockers to isolate certain types of voltage-activated currents).</li>
</ol>
2. Workspace Preparation
<ol>
	<li>Fill the oxygenating slice storing chamber with S2 at least 30 min prior to dissection, place the slice on ice for temperature and pH adjustment, and oxygenate the solution continuously.</li>
	<li>Fill the reservoir for slice superfusion at recording setup with S2 and oxygenate continuously.</li>
	<li>Prior to dissection, fill the vibratome chamber with S2 and arrange crushed ice around the chamber. Alternatively, transfer the spare ice-cold oxygenated solution from the oxygenating chamber into the vibratome chamber and keep oxygenating continuously.</li>
	<li>Arrange surgical tools and consumables.</li>
	<li>Place the ice gel pack under the dissecting microscope and cover it with a paper towel to prevent the VNO tissue from freezing to the bottom of the dish.</li>
	<li>Clean the razor blade by briefly rinsing it in 70% ethanol and distilled water, then mounting it to the vibratome. Replace it for every slicing session.</li>
</ol>
3. VNO Dissection and Embedding
<ol>
	<li>Sacrifice the animal by brief exposure to CO2 and decapitate it using sharp surgical scissors. Note: As time from sacrificing the animal to putting the VNO capsule on ice is critical, minimize the time to less than 2 min. To maintain tissue viability, embed both fully dissected VNOs in agarose in less than 30 min.</li>
	<li>Remove the lower jaw with large surgical scissors. Enter through the mouth cavity and cut the mandible bones and muscles of each side separately.</li>
	<li>Place the remaining part of the head upside down in the large Petri dish.</li>
	<li>Pull away the skin of the upper jaw and around the tip of the nose with medium forceps to gain better access to the incisors.</li>
	<li>Use bone scissors to cut away the largest part of the incisors at a ~45&#176; angle in the rostral direction (Figure 1A). This will ease the removal of the VNO capsule from the nasal cavity. 
	Note: Do not cut to the root of the tooth to prevent damage to the tip of the VNO capsule.</li>
	<li>Grab the rigid upper palate at its rostral part with medium forceps and carefully peel back in one piece at a flat angle (Figure 1B). 
	Note: Repeatedly rinse with ice-cold S2.</li>
	<li>Use microspring scissors to cut the bony fusion between the tip of the vomer bone and the jaw. Insert the scissor tips with the curved part of the tip pointing outward away from the VNO and carefully cut the bone in small steps on both the left and right sides lateral to the VNO capsule.</li>
	<li>To remove the VNO capsule, use micro spring scissors to cut through the vomer bone at the caudal part and carefully lift it out of the nasal cavity using medium forceps. Immediately transfer the VNO to a small petri dish under a stereo microscope on an ice gel pack, where the remaining steps of the dissection will be performed.</li>
	<li>Rinse the VNO in a small amount of ice-cold S2 to prevent the tissue from drying out.</li>
	<li>Separate the cartilaginous capsules that contain the VNO soft tissues by grabbing the back of the vomer bone with medium forceps. Position the capsule for a dorsal view so that a split between both VNOs becomes visible (Figure 1Di).</li>
	<li>Use the tip of fine forceps to separate both cartilage VNO capsules from the central bone while keeping the vomer bone pinned down at the rear part. 
	Note: Use forceps only at the rim of the cartilage capsule, and be very careful not to pierce through the cartilage as the delicate sensory epithelium is easily damaged.</li>
	<li>Once the two VNOs are separated, start removing the cartilage encapsulating the first VNO.</li>
	<li>Grab the top rim of the capsule with one fine forceps and split away the cartilage wall that was previously attached to the vomer bone (medial side).</li>
	<li>To remove the remaining cartilage, turn the VNO with its curved lateral side to the bottom of the dish and securely pin down the cartilage on one side using forceps. Carefully move the second fine forceps from the back side at a very flat angle between the cartilage and VNO to loosen the connection between tissue and cartilage.</li>
	<li>To avoid damaging the sensory epithelium, slowly peel the VNO away from the cartilage by holding it at its caudal tip.</li>
	<li>Once the VNO is levered from the capsule, remove all remaining small cartilage parts. Any remaining pieces of cartilage will detach the tissue from the surrounding agarose during the slicing process.</li>
	<li>Place a small drop of ice-cold S2 on the first dissected VNO to prevent tissue damage. A large blood vessel on the lateral side will become visible, indicating that the organ is still intact and was not grossly damaged during the dissection. In case the blood vessel got damaged, it will still be worthwhile to carry on with slicing the VNO as long as the overall morphology was not clearly impaired.</li>
	<li>Immediately dissect the second VNO.</li>
	<li>To embed the VNOs, fill both small Petri dishes to the rim with melted S3 (stored in a water bath at 42 &#176;C; see 1.3).</li>
	<li>Hold the VNO on the broader caudal end with fine forceps to avoid damage to the sensory epithelium.</li>
	<li>Immerse the VNO in the agarose and move it horizontally back and forth several times to remove the film of the extracellular solution as well as any air bubbles from its surface.</li>
	<li>Position the VNO vertically, with the caudal tip facing the bottom of the dish. Instead of directly pinching the VNO with the forceps, move the forceps tip in close proximity to the VNO to adjust orientation. 
	Note: Orientation during embedding is crucial as it determines slice plane and accessibility to sensory neurons during the experiment.</li>
	<li>Place dishes on a gel ice pack and wait until the agarose has solidified. 
	Note: Do not change VNO orientation once the agarose solidifies, as this will detach the tissue from the surrounding agarose.</li>
</ol>
4. Coronal VNO Tissue Slicing
<ol>
	<li>Use a small spatula to remove the agarose block from the small dish into the lid of a large Petri dish. Flip the agarose upside down, leaving the caudal tip of the VNO facing upwards.</li>
	<li>Cut the block into a pyramidal shape using a surgical scalpel (3-4 mm at the tip, 8-10 mm at the bottom). Take care not to damage the embedded tissue.</li>
	<li>Use super glue to fix the pyramid-shaped block to the center of the vibratome specimen plate and wait ~1 min for the glue to dry completely.</li>
	<li>Transfer the specimen plate to the slicing chamber and prepare the second VNO accordingly. Keep a plate with the second specimen at 4 &#176;C until use.</li>
	<li>Use a vibrating blade microtome with the following settings: thickness: 150-200 &#181;m; speed: 3.5 a.u. = 0.15 mm/sec; frequency: 7.5 a.u. = 75 Hz. Transfer slices to an oxygenating chamber until use after briefly inspecting slice morphology under the dissecting microscope. Slices can be kept for several hours.</li>
</ol>

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Agarose (low-gelling temperature)</td>
			<td>PeqLab</td>
			<td>35-2030</td>
			<td></td>
		</tr>
		<tr>
			<td>ATP (Mg-ATP)</td>
			<td>Sigma-Aldrich</td>
			<td>A9187</td>
			<td></td>
		</tr>
		<tr>
			<td>Bis(2-hydroxyethyl)-2-aminoethanesulfonic acid (BES)</td>
			<td>Sigma-Aldrich</td>
			<td>B9879</td>
			<td></td>
		</tr>
		<tr>
			<td>Calcium chloride</td>
			<td>Sigma-Aldrich</td>
			<td>C1016</td>
			<td></td>
		</tr>
		<tr>
			<td>Ethylene glycol tetraacetic acid (EGTA)</td>
			<td>Sigma-Aldrich</td>
			<td>E3889</td>
			<td></td>
		</tr>
		<tr>
			<td>Glucose</td>
			<td>Sigma-Aldrich</td>
			<td>G8270</td>
			<td></td>
		</tr>
		<tr>
			<td>GTP (Na-GTP)</td>
			<td>Sigma-Aldrich</td>
			<td>51120</td>
			<td></td>
		</tr>
		<tr>
			<td>(2-hydroxyethyl)-1-piperazineethanesulfonic acid (HEPES)</td>
			<td>Sigma-Aldrich</td>
			<td>H3375</td>
			<td></td>
		</tr>
		<tr>
			<td>Magnesium chloride</td>
			<td>Sigma-Aldrich</td>
			<td>M8266</td>
			<td></td>
		</tr>
		<tr>
			<td>Potassium chloride</td>
			<td>Sigma-Aldrich</td>
			<td>P9333</td>
			<td></td>
		</tr>
		<tr>
			<td>Potassium hydroxide</td>
			<td>Sigma-Aldrich</td>
			<td>3564</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium chloride</td>
			<td>Sigma-Aldrich</td>
			<td>S7653</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium hydrogen carbonate</td>
			<td>Sigma-Aldrich</td>
			<td>S5761</td>
			<td></td>
		</tr>
		<tr>
			<td>Sodium hydroxide</td>
			<td>Sigma-Aldrich</td>
			<td>S8045</td>
			<td></td>
		</tr>
		<tr>
			<td>Large petri dish, 90 mm</td>
			<td>VWR</td>
			<td></td>
			<td>decapitation, dissection of VNO capsule</td>
		</tr>
		<tr>
			<td>Small petri dish, 35 mm</td>
			<td>VWR</td>
			<td></td>
			<td>lid for VNO dissection, dish for embedding in agarose</td>
		</tr>
		<tr>
			<td>Sharp large surgical scissor</td>
			<td>Fine Science Tools</td>
			<td></td>
			<td>decapitation, removal of lower jaw</td>
		</tr>
		<tr>
			<td>Strong bone scissors</td>
			<td>Fine Science Tools</td>
			<td></td>
			<td>cutting incisors</td>
		</tr>
		<tr>
			<td>Medium forceps, Dumont tweezers #2</td>
			<td>Fine Science Tools</td>
			<td></td>
			<td>removing skin and palate</td>
		</tr>
		<tr>
			<td>Micro spring scissors, 8.5 cm, curved, 7 mm blades</td>
			<td>Fine Science Tools</td>
			<td></td>
			<td>cutting out VNO</td>
		</tr>
		<tr>
			<td>Two pairs of fine forceps, Dumont tweezers #5</td>
			<td>Fine Science Tools</td>
			<td></td>
			<td>dissecting VNO out of cartilaginous capsule</td>
		</tr>
		<tr>
			<td>Small stainless steel spatula</td>
			<td>Fine Science Tools</td>
			<td></td>
			<td>handling agarose block and tissue slices</td>
		</tr>
		<tr>
			<td>Hot plate magnetic stirrer</td>
			<td>Snijders</td>
			<td>34532</td>
			<td></td>
		</tr>
		<tr>
			<td>Microforge</td>
			<td>Narishige</td>
			<td>MF-830</td>
			<td></td>
		</tr>
		<tr>
			<td>pH Meter five easy</td>
			<td>Mettler Toledo</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Pipette storage jar</td>
			<td>World Precision Instruments</td>
			<td>e212</td>
			<td></td>
		</tr>
		<tr>
			<td>Razor blades</td>
			<td>Wilkinson Sword GmbH</td>
			<td>Wilkinson Sword Classic</td>
			<td></td>
		</tr>
		<tr>
			<td>Oxygenating slice storage chamber; alternative commercial chambers are e.g. BSK1 Brain Slice Keeper (Digitimer) or the Pre-chamber (BSC-PC; Warner Instruments)</td>
			<td>custom-made</td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Stereo microscope</td>
			<td>Leica Microsystems</td>
			<td>S4E</td>
			<td></td>
		</tr>
		<tr>
			<td>Vibratome</td>
			<td>Leica Microsystems</td>
			<td>VT 1000 S</td>
			<td></td>
		</tr>
		<tr>
			<td>Water bath</td>
			<td>Memmert</td>
			<td>WNB 45</td>
			<td></td>
		</tr>
	</tbody>
</table>

preparation of mouse vomeronasal organ for vibratome sectioning

Source: Ackels, T., et al. <a href="https://app.jove.com/v/54517">In-depth physiological analysis of defined cell populations in acute tissue slices of the mouse vomeronasal organ.</a> J. Vis. Exp. (2016)
This video outlines the isolation of a mouse vomeronasal organ (VNO) and tissue preparation for vibratome sectioning. Sections are used to characterize the biophysical and physiological attributes of a specific group of sensory neurons.

<img alt="Figure 1" src="/files/ftp_upload/22622/22622_figure_1.jpg" /> 
Figure 1: Dissection of the VNO. (A) Side view on the mouse head to illustrate the position and angle at which the incisors are cut. (B) Ventral view depicting the best point to grab and peel back the upper palate (UP). (C) Ventral view onto the cartilage capsule (CC) that harbors the VNO and the vomer bone (VB) after removing the lower jaw, incisors and palate. (D) Dorsal view of the dissected VNO capsule depicting the bilateral localization of both VNOs (Di). The lateral view illustrates the rim of cartilage on the dorsal side where both VNOs need to be separated (Dii). Scale bar = 1 mm (A-D).

Preparation of Mouse Vomeronasal Organ for Vibratome Sectioning

All procedures involving animal models have been reviewed by the local institutional animal care committee and the JoVE veterinary review board.
Both ...

Begin with a mouse vomeronasal organ, or VNO, located at the base of the nasal septum.
This contains a thin layer of tissue harboring special smell-sensing neurons that detect pheromones.
Add a drop of cold solution to the VNO to prevent drying.
Separate each VNO capsule from the bony tissue and the central bone.
Remove the surrounding cartilaginous capsule.
Transfer the VNO to a cold surface and add a drop of cold solution to minimize tissue damage.
Immerse the VNO in molten agarose, move it to remove excess solution, then, position the VNO vertically. Place on ice to solidify the agarose and embed the VNO.
Invert the solidified agarose and trim it to the desired shape.
Fix the blocks on a specimen plate.
Now, section the tissue using a vibratome.
Store the sections in an oxygenated chamber containing a pH-adjusted solution to maintain cell activity for further studies.

preparation-of-mouse-vomeronasal-organ-for-vibratome-sectioning

Nanyang Technological University

Research

JoVE Encyclopedia of Experiments

Neuroscience

Neuronal Culture Techniques

Primary Neuronal Culture

65 Views. Source: Ackels, T., et al. In-depth physiological analysis of defined cell populations in acute tissue slices of the mouse vomeronasal organ. J. Vis. Exp. (2016) This video outlines the isolation of a mouse vomeronasal organ (VNO) and tissue preparation for vibratome sectioning. Sections are used to characterize the biophysical and physiological attributes of a specific group of sensory neurons. 

Video: Preparation of Mouse Vomeronasal Organ for Vibratome Sectioning - Concept

Ex Vivo Preparations of the Intact Vomeronasal Organ and Accessory Olfactory Bulb

The mouse accessory olfactory system (AOS) is a specialized sensory pathway for detecting nonvolatile social odors, pheromones, and kairomones. The first neural circuit in the AOS pathway, called the accessory olfactory bulb (AOB), plays an important role in establishing sex-typical behaviors such as territorial aggression and mating. This small (&#60;1 mm3) circuit possesses the capacity to distinguish unique behavioral states, such as sex, strain, and stress from chemosensory cues in the secretions and excretions of conspecifics. While the compact organization of this system presents unique opportunities for recording from large portions of the circuit simultaneously, investigation of sensory processing in the AOB remains challenging, largely due to its experimentally disadvantageous location in the brain. Here, we demonstrate a multi-stage dissection that removes the intact AOB inside a single hemisphere of the anterior mouse skull, leaving connections to both the peripheral vomeronasal sensory neurons (VSNs) and local neuronal circuitry intact. The procedure exposes the AOB surface to direct visual inspection, facilitating electrophysiological and optical recordings from AOB circuit elements in the absence of anesthetics. Upon inserting a thin cannula into the vomeronasal organ (VNO), which houses the VSNs, one can directly expose the periphery to social odors and pheromones while recording downstream activity in the AOB. This procedure enables controlled inquiries into AOS information processing, which can shed light on mechanisms linking pheromone exposure to changes in behavior.

Ex Vivo Preparations of the Intact Vomeronasal Organ and Accessory Olfactory Bulb

The mouse accessory olfactory bulb (AOB) has been difficult to study in the context of sensory coding. Here, we demonstrate a dissection that produces an ex vivo preparation in which AOB neurons remain functionally connected to their peripheral inputs, facilitating research into information processing of mouse pheromones and kairomones.

The mouse accessory olfactory system (AOS) is a specialized sensory pathway for detecting nonvolatile social odors, pheromones, and kairomones. The first ...

JoVE Journal

Preparation of Acute Brain Slices Using an Optimized N-Methyl-D-glucamine Protective Recovery Method

This protocol is a practical guide to the N-methyl-D-glucamine (NMDG) protective recovery method of brain slice preparation. Numerous recent studies have validated the utility of this method for enhancing neuronal preservation and overall brain slice viability. The implementation of this technique by early adopters has facilitated detailed investigations into brain function using diverse experimental applications and spanning a wide range of animal ages, brain regions, and cell types. Steps are outlined for carrying out the protective recovery brain slice technique using an optimized NMDG artificial cerebrospinal fluid (aCSF) media formulation and enhanced procedure to reliably obtain healthy brain slices for patch clamp electrophysiology. With this updated approach, a substantial improvement is observed in the speed and reliability of gigaohm seal formation during targeted patch clamp recording experiments while maintaining excellent neuronal preservation, thereby facilitating challenging experimental applications. Representative results are provided from multi-neuron patch clamp recording experiments to assay synaptic connectivity in neocortical brain slices prepared from young adult transgenic mice and mature adult human neurosurgical specimens. Furthermore, the optimized NMDG protective recovery method of brain slicing is compatible with both juvenile and adult animals, thus resolving a limitation of the original methodology. In summary, a single media formulation and brain slicing procedure can be implemented across various species and ages to achieve excellent viability and tissue preservation.

Preparation of Acute Brain Slices Using an Optimized N-Methyl-D-glucamine Protective Recovery Method

This protocol demonstrates the implementation of an optimized N-methyl-D-glucamine (NMDG) protective recovery method of brain slice preparation. A single media formulation is used to reliably obtain healthy brain slices from animals of any age and for diverse experimental applications.

This protocol is a practical guide to the N-methyl-D-glucamine (NMDG) protective recovery method of brain slice preparation. Numerous recent studies have ...

Quadruple Immunostaining of the Olfactory Bulb for Visualization of Olfactory Sensory Axon Molecular Identity Codes

The mouse olfactory system is often used to study mechanisms of neural circuit formation&#12288;because of its simple anatomical structure. An Olfactory Sensory Neuron (OSN) is a bipolar cell with a single dendrite and a single unbranched axon. An OSN expresses only one Olfactory Receptor (OR) gene, OSNs expressing a given type of OR converge their axons to a few sets of invariant glomeruli in the Olfactory Bulb (OB). A remarkable feature of OSN projection is that the expressed ORs play instructive roles in axonal projection. ORs regulate the expression of multiple axon-sorting molecules and generate the combinatorial molecular code of axon-sorting molecules at the OSN axon termini. Thus, to understand the molecular mechanisms of OR-specific axon guidance mechanisms, it is vital to characterize their expression profiles at the OSN axon termini within the same glomerulus. The aim of this article was to introduce methods for collecting as many glomeruli as possible on a single OB section and for performing immunostaining using multiple antibodies. This would allow the comparison and analysis of the expression patterns of axon-sorting molecules without staining variation between OB sections.

Olfactory sensory neurons express a wide variety of axon-sorting molecules to establish proper neural circuitry. This protocol describes an immunohistochemical staining method to visualize combinatorial expressions of axon-sorting molecules at the axon termini of olfactory sensory neurons.

The mouse olfactory system is often used to study mechanisms of neural circuit formation&#12288;because of its simple anatomical structure. An Olfactory ...

Preparation of Mouse Vomeronasal Organ for Vibratome Sectioning

Transcript

Preparation of Mouse Vomeronasal Organ for Vibratome Sectioning

Ex Vivo Preparations of the Intact Vomeronasal Organ and Accessory Olfactory Bulb

Preparation of Acute Brain Slices Using an Optimized N-Methyl-D-glucamine Protective Recovery Method

Quadruple Immunostaining of the Olfactory Bulb for Visualization of Olfactory Sensory Axon Molecular Identity Codes