The authors acknowledge technical or editorial assistance from Taylor Wilt (Xona), Smita Paranjape (UNC-Chapel Hill), Joyce Ciechanowski (Xona) and Brad Taylor (Xona). The authors acknowledge support from Xona Microfluidics, LLC and the National Institute of Mental Health (R42 MH097377). Imaging was partially supported by the Confocal and Multiphoton Imaging Core Facility of NINDS Center Grant P30 NS045892 and NICHD Center Grant (U54 HD079124). The content is solely the responsibility of the authors and does not necessarily represent the official views of the National Institutes of Health.

NOTE: A schematic of the plastic multicompartment chip is shown in Figure 1A, B. The chip is the size of a standard microscope slide (75 mm &#215; 25 mm). The features of the chip, including main channels or compartments, wells, and microgrooves are labeled and are provided for future reference. Figure 1C is a photograph of the chip demonstrating the fluidic isolation of the compartments.
1. Preparation and Coating of the Multicompartment Chips
<ol>
	<li>In a bio-safety cabinet, place the chip into a Petri dish or other suitable sterile container.</li>
	<li>Add 100 &#181;L of pre-coating solution to the upper left well of the chip and allow it to flow through the main channel into the adjoining well. 
	NOTE: The pre-coating solution is used to pre-coat the microfluidic channels to eliminate the potential for trapping air bubbles within the chip.</li>
	<li>Fill the lower left well with 100 &#181;L of pre-coating solution. Wait 5 min to allow the solution to flow through the microgrooves.</li>
	<li>Add 100 &#181;L of pre-coating solution to the upper right well and allow it to flow through the main channel into the adjoining well. Fill the lower right well with 100 &#181;L of pre-coating solution.</li>
	<li>Aspirate the solution from each well. Aspirate away from the main channels to avoid removing liquid from the main channels (Figure 2A). Immediately add 150 &#181;L of phosphate-buffered saline (PBS) to the upper left well. Wait 1.5 min. 
	CAUTION: Do not aspirate all liquid from the enclosed main channels.</li>
	<li>Add 150 &#181;L PBS to the lower left well. Wait 5 min to allow liquids to flow through the microgrooves. Add 150 &#181;L PBS to the upper right well. Add 150 &#181;L PBS to lower right well. Wait 10 min.</li>
	<li>Repeat steps 1.5-1.6 for a second PBS wash.</li>
	<li>Check the chip under a tissue culture microscope for bubbles in the main channels. If bubbles are present, perform the procedures below. If no bubbles are present, skip to step 1.9.
	<ol>
		<li>Aspirate PBS from the wells angling the pipet tip away from the channel opening (Figure 2A).</li>
		<li>Dispense 100 &#181;L of pre-coating solution into the upper well, angling the tip of the pipet near the channel opening (Figure 2B). The bubbles should move through the channel into the lower well. Wait 1.5 min.</li>
		<li>Repeat steps 1.3-1.8.</li>
	</ol>
	</li>
	<li>Aspirate PBS from the wells angling the pipet tip away from the channel opening (Figure 2A).</li>
	<li>Add 100 &#181;L of 0.5 mg/mL poly d-lysine (PDL) to the upper left well of the chip. Wait 1.5 min. Fill the lower left well with 100 &#181;L of PDL.</li>
	<li>Add 100 &#181;L of PDL to the upper right well of the chip. Wait 1.5 min. Add 100 &#181;L to the lower right well.</li>
	<li>Close the petri dish&#160;and place the chip in an incubator at 37 &#176;C for 1 h.</li>
	<li>Repeat PBS wash steps 1.5-1.6 twice to remove excess PDL.</li>
	<li>Aspirate the PBS from the device.</li>
	<li>Immediately add 100 &#181;L of cell culture media to the upper left well of the chip. Wait 1.5 min. Add media to the lower left well. Add media to the upper right well. Wait 1.5 min. Add 100 &#181;L medium to the lower right well of the chip.</li>
	<li>Place the chip in the 37&#176;C incubator until ready to plate cells.</li>
</ol>
2. Seeding Neurons into the Multicompartment Chips
<ol>
	<li>Prepare cell suspension of dissociated rat hippocampal neurons according to established protocols21,22 to yield a density of ~12 &#215; 106 cells/mL. 
	NOTE: Use of cell suspension densities between 3 and 12 &#215; 106 cells/mL is possible. If a lower density is used, the volume of cell suspension to be added to the chip may be increased (see below). The procedure described below is applicable for murine dissociated cortical or hippocampal neurons. Optimal cell densities for other neuron types may vary.</li>
	<li>Remove the majority of media in each well of the chip, leaving approximately 5&#160;&#181;L in each well. Aspirate away from the main channels to avoid removing liquid from the main channels (Figure 2A). 
	CAUTION: Do not aspirate liquid from the enclosed main channels. Air bubbles may become trapped in the chip if fluid is aspirated from the main channels.</li>
	<li>Load 5 &#181;L of cell suspension in the upper right well and another 5 &#181;L of cell suspension in the lower right well (~120,000 cells total). Load the cells by dispensing close to the main channel (Figure 2B). Check under a microscope to ensure the neurons are in the main channel. Wait for 5 min to allow the cells to attach. 
	NOTE: Neurons can be loaded into either compartment. For explanation purposes, the somatic compartment is the main channel on the right side, but either compartment can be used as the somatic compartment. Use of lower cell densities down to 60,000 cells per chip is possible. Up to 10 &#181;L of cell suspension may be added to each well of the somatic compartment in combination with a cell suspension with fewer cells than described above.</li>
	<li>Add approximately 150 &#181;L of neuronal culture media to each of the upper and lower right wells, and then add 150 &#181;L of media to each of the upper and lower left wells. Place the chip into humidified tray in a 5% CO2 37 &#176;C incubator.</li>
	<li>After 24 h, perform a media change by removing media from the wells. Make sure the main channel remains filled. Add 150 &#181;L of media to each top well, and then fill the bottom wells.</li>
	<li>Place the chip back in the incubator for the desired number of days. 
	NOTE: Monitor the media every couple of days to make sure it remains light pink. If the media is yellowish, replace 50% of it with fresh media. If the fluid level is low, make sure there is adequate humidity and appropriate secondary containment of the chips to prevent evaporation. Minimizing, or even eliminating, media changes is possible using secondary containment and/or covering the dish containing the chip with polytetrafluoroethylene (PTFE)-FEP film.</li>
</ol>
3. Retrograde Labeling of Neurons within the Chip
NOTE: Retrograde labeling can be performed using multiple techniques, including using modified cholera toxin and rabies virus. Below are instructions for labeling neurons using G-deleted Rabies-mCherry or -eGFP virus. Handle potentially infectious materials according to the local organization&#39;s guidelines. Additional training may be required.
<ol>
	<li>Warm fresh neuronal culture media to 37 &#176;C. Estimate ~400 &#181;L of media per chip.</li>
	<li>Dilute 100,000 viral units of modified rabies virus in a total of 50 &#181;L using media taken from either well of the axonal compartment. 
	NOTE: Dispose of tips and tubes in contact with the virus according to the organization-approved protocol.</li>
	<li>Gently pipet the remaining media from the wells of the axonal compartment and store in a centrifuge tube at 37 &#176;C.</li>
	<li>Add 150 &#181;L of fresh warm media and the 50 &#181;L of diluted virus to the axonal compartment. Incubate for 2 h at 37 &#176;C incubator.</li>
	<li>Remove media containing virus and dispose of it properly. 
	NOTE: Air bubbles may become trapped in the chip if fluid is aspirated from the main channels.</li>
	<li>Gently add 75 &#181;L of fresh media to one axon well and allow it to flow to the other axon well.</li>
	<li>Remove flow-through from the second axon well and dispose properly.</li>
	<li>Repeat steps 3.6 and 3.7 once.</li>
	<li>Add back stored media to the axonal compartment. Add approximately 50 &#181;L fresh media, if necessary, to maintain adequate volume and return the cells to the incubator. 
	NOTE: Fluorescent protein expression is visible by 48 h and persists for up to 8 days. Neurons can be imaged for up to 30 min at room temperature in neuronal culture media. Culture media can also be replaced with warmed CO2-independent hibernate E with B27 and imaged for longer. Neurons can also be imaged within a well-humidified environmental chamber at 37 &#176;C and 5% CO2. In this case, humidification is critical for minimizing evaporative losses within the chips, which is exacerbated by heating and can compromise neuron health.</li>
</ol>
4. Fluidic Isolation of the Axonal Compartment within the Chip
<ol>
	<li>Remove 20 &#181;L from the lower left well of the axonal compartment and place into the upper right well of the somatic compartment. Wait 2 min for flow within each channel to equilibrate.</li>
	<li>Remove 50 &#181;L of media from the axonal compartment. Add 0.3 &#181;L of 1 mM Alexa Fluor 488 hydrazide to this media, mix via pipet and return back to the axonal compartment. The chip is ready for imaging. 
	NOTE: Other compounds of interest can be added. Adding a fluorescent dye with a similar molecular weight as the compound of interest is recommended in order to monitor fluidic isolation over time.</li>
</ol>
5. Performing Axotomy Within the Chip
<ol>
	<li>Remove media from the axonal compartment keeping the pipet tip away from the entrance of the main channel (Figure 2A) and store it in a centrifuge tube.</li>
	<li>Aspirate the axonal compartment completely, placing the aspiration pipet near either entrance of the main channel of the axonal compartment (Figure 2B). Continue aspiration for 1-2 min. Make sure that solution is completely removed from the compartment. 
	NOTE: The vacuum pressure for aspiration must be at least 18 inch-Hg for the axotomy procedure to work properly.</li>
	<li>Replace the axonal compartment with the stored media and confirm that the axons are&#160; severed by looking at the chip under a microscope. 
	NOTE: If bubbles form in the axonal compartment when replacing the media, repeat steps 5.1-5.2.</li>
	<li>Return the chip to the incubator.</li>
</ol>
6. Fluorescence Immunostaining within the Chip
<ol>
	<li>Prepare 4% formaldehyde fixation solution in PBS (4% formaldehyde, 1 &#181;M MgCl2, 0.1 &#181;m CaCl2, 120 mM sucrose)</li>
	<li>Remove most of the media in the wells of the chip (do not dry interior compartments).</li>
	<li>Immediately add 100 &#181;L of fixation solution to the top wells of the axonal and somatic compartments.</li>
	<li>After 1 min, add 100 &#181;L of fixation solution to the bottom wells. Fix for 30 min at room temperature.</li>
	<li>Remove most of the solution from the wells of the chip (do not dry interior compartments). Immediately add 150 &#181;L of PBS to each of the top wells of the axonal and somatic compartments. Wait 2 min for the PBS to flow into the bottom wells.</li>
	<li>Repeat step 6.5 twice.</li>
	<li>Remove most of the PBS from the wells of the chip. Immediately add 150 &#181;L of PBS with 0.25% TritonX-100 to each of the top wells of the axonal and somatic compartments. Wait for 15 min.</li>
	<li>Remove most of the liquid from the wells of the chip and immediately add 150 &#181;L of blocking solution (10% normal goat serum in PBS) to each of the top wells of the axonal and somatic compartments. Wait for 15 min. 
	NOTE: Effective blocking solutions should be specific to the secondary antibody, e.g., for a donkey anti-sheep secondary antibody, use donkey serum in the blocking solution.</li>
	<li>Remove most of the liquid from the wells of the chip and immediately add 100 &#181;L of primary antibody (or antibodies) in 1% normal goat serum in PBS to each of the top wells of the axonal and somatic compartments. Cover to minimize evaporation and wait for 1 h at room temperature or 4 &#176;C overnight.</li>
	<li>Remove most of the solution from the wells of the chip (do not dry interior compartments). Immediately add 150 &#181;L of PBS to each of the top wells of the axonal and somatic compartments. Wait 5 min for the PBS to flow into the bottom wells.</li>
	<li>Repeat step 6.10 twice.</li>
	<li>Remove most of the liquid from the wells of the chip and immediately add 100 &#181;L of secondary antibody (or antibodies) in PBS to each of the top wells of the axonal and somatic compartments. Cover to minimize evaporation and wait for 1 h at room temperature. 
	NOTE: Refer to the manufacturer&#39;s instructions for the recommended dilution of secondary antibodies.</li>
	<li>Repeat steps 6.10-6.11.</li>
	<li>If imaging within 1 day of immunostaining, keep the chip filled with PBS. If chip will be stored longer than 1 day before imaging, wrap the dish containing the chip in paraffin film to prevent evaporation and store at 4 &#176;C until ready to image.</li>
	<li>For longer term storage of samples, mounting media (e.g., Fluoromount-G) can be used.
	<ol>
		<li>Remove most of the liquid from the wells of the chip. Use a 1 mL disposable plastic pipet to add 2 drops of mounting media to each of the top wells of the axonal and somatic compartments.</li>
		<li>Tilt the chip to encourage the flow of the mounting media through the channels. After 5 min add 2 drops to the bottom wells. Wait for 1 h before imaging. 
		NOTE: After using mounting media it will not be possible to re-probe for other targets.</li>
	</ol>
	</li>
</ol>

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A.M.T. is an inventor of the microfluidic chamber/chip (US 7419822 B2) and is a member of Xona Microfluidics, LLC. V.P. is an employee of Xona Microfluidics, LLC. J.H. is a member of Xona Microfluidics, LLC. T.N. declares no competing financial interests.&#160;Open access publication of this article is sponsored by Xona Microfluidics.

Plastic multicompartment chips provide an easy-to-use option for compartmentalizing neurons, providing long-term neuronal cultures (&gt;3 weeks). This protocol details how to culture cortical and hippocampal murine neurons within these chips. The creation of soluble microenvironments and how to retrograde label neurons, perform axotomy, and perform immunocytochemistry were also discussed. Importantly, these chips are compatible with high-resolution, fluorescence, and live imaging. 
Plastic multicompartment chips provide many of the same functions as the PDMS-based compartmentalized devices, but have advantages, disadvantages, and some distinguishing features. Table 1 provides a feature comparison of both plastic chip and PDMS-based devices. First and foremost, the chips are pre-assembled and made permanently hydrophilic, which facilitates wetting, making them easier to use. The plastic is not gas permeable, unlike PDMS, so if bubbles unexpectedly form within the channels, they do not readily escape and must be removed. A pre-coating solution containing mainly ethanol and some other proprietary agents eliminates bubble formation. 
Live imaging of projections following transduction of fluorescent proteins was performed within the chips (Figure 4) and there was no detectable autofluorescence of the plastic. A caveat is that immersion oils used with the chip for high numerical aperture objectives must be silicone oil based, and not mineral oil based. Mineral oil can cause an adverse reaction with the cyclic olefin copolymer. For brightfield imaging, it is important to note that the microgrooves in the chip are rounded at the ends and there is a gradual tapering of the z-direction of the main channels towards the microgroove barrier causing some light refraction at either end of the microgrooves during brightfield imaging (Figure 3). Because the chip is pre-assembled, antibody penetration into the micron-sized microgrooves may be uneven (as with permanently bonded PDMS-based devices); thus, quantitative analysis following immunostaining should be performed in the channels/compartments. Immunostaining of neuronal projections within the microgrooves can be improved by creating a volume difference between the compartments to aid the flow of antibodies and fluorophores into the microgrooves.

Traditional neuron culture approaches result in random outgrowth of axons and dendrites, which prevent the study of neurons in their unique polarized morphology. Microfabricated multicompartment devices have become well-established and well-used research tools for neuroscientists in the last 10-15 years (selected high-profile publications are referenced1,2,3,4,5,6,7,8,9,10,11,12,13,14,15,16,17). These devices compartmentalize neurons and provide a method to physically and chemically manipulate subcellular regions of neurons, including somata, dendrites, axons, and synapses18,19. They also provide multiple experimental paradigms that are not possible using random cultures, including studies of axonal transport, axonal protein synthesis, axon injury/regeneration, and axon-to-soma signaling. The basic 2-compartment configuration consists of two parallel microfluidic channels separated by a series of smaller perpendicular microgrooves. Primary or stem cell-derived neurons are plated into one of the microfluidic channels, settle and attach to the bottom surface of the device, and extend neurites over the course of days. Many growth cones find their way into the microgrooves, which are small enough that they prevent cell bodies from entering. Because growth cones are physically restricted and unable to turn around within the microgrooves, they grow straight into the adjacent compartment (axonal compartment) where they are isolated.
Historically, these devices have been molded using poly(dimethylsiloxane) (PDMS) from a photolithographically patterned master mold and are either made in-house in investigators&#39; laboratories or purchased commercially. One of the main drawbacks of using PDMS is its hydrophobicity20. PDMS can be made hydrophilic temporarily, but then quickly becomes hydrophobic within hours in a non-aqueous environment20. Because of this, the devices must be attached to a glass coverslip or other suitable substrate at the time of use. Pre-assembled plastic multicompartment chips are now commercially available (e.g., XonaChips) in injection molded plastic. These chips are made permanently hydrophilic, simplifying device wetting and allowing the pre-assembly of the chip with a thin film of cyclic olefin copolymer (COC) enclosing the microfluidic channels on the bottom. These chips are fabricated in an optically transparent plastic suitable for high-resolution fluorescence imaging.
The purpose of this protocol is to demonstrate the use of the pre-assembled plastic microfluidic chips for multiple experimental paradigms performed using murine hippocampal or cortical neurons. This protocol describes how to retrograde label neurons using a modified rabies virus within the chip. Axotomy for studies of axon injury and regeneration are also described. Lastly, this protocol shows how to perform fluorescence immunostaining with the device.

<table border="0" cellpadding="0" cellspacing="0" style="width:652px;" width="651">
	<tbody>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">XonaChip</td>
			<td style="width:175px;">Xona Microfluidics, LLC</td>
			<td style="width:109px;">XC150</td>
			<td style="width:165px;">150 &#181;m length microgroove barrier</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;"></td>
			<td style="width:175px;">Xona Microfluidics, LLC</td>
			<td style="width:109px;">XC450</td>
			<td style="width:165px;">450 &#181;m length microgroove barrier</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;"></td>
			<td style="width:175px;">Xona Microfluidics, LLC</td>
			<td style="width:109px;">XC900</td>
			<td style="width:165px;">900 &#181;m length microgroove barrier</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">XC pre-coat&#160;</td>
			<td style="width:175px;">Xona Microfluidics, LLC</td>
			<td style="width:109px;">XC Pre-Coat</td>
			<td style="width:165px;">included with XonaChips</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">XonaPDL&#160;</td>
			<td style="width:175px;">Xona Microfluidics, LLC</td>
			<td style="width:109px;">XonaPDL</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">E17/E18 timed pregnant Sprague Dawley rats</td>
			<td style="width:175px;">Charles River</td>
			<td style="width:109px;">24100564</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">neuronal culture media:</td>
			<td style="width:175px;"></td>
			<td style="width:109px;"></td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">- Neurobasal medium</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">21103049</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">-B-27 Plus Supplement (50x)</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">A3582801</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">-GlutaMAX Supplement</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">35050061</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">-Antibiotic-Antimycotic (100x)</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">15240112</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">fluorinated ethylene propylene film</td>
			<td style="width:175px;">American Durafilm</td>
			<td style="width:109px;">50A</td>
			<td style="width:165px;">0.5 mil thickness</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">modified rabies virus</td>
			<td style="width:175px;">Salk Institute for Biological Studies</td>
			<td style="width:109px;">G-deleted Rabies-eGFP</td>
			<td style="width:165px;">Material Transfer Agreement required</td>
		</tr>
		<tr height="63">
			<td height="63" style="height:63px;width:203px;"></td>
			<td style="width:175px;">Salk Institute for Biological Studies</td>
			<td style="width:109px;">G-deleted Rabies-mCherry</td>
			<td style="width:165px;">Material Transfer Agreement required</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">Alexa Fluor hydrazide 488</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">A10436</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">Fluoromount G</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">00-4958-02</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">Glass Pasteur pipettes</td>
			<td style="width:175px;">Sigma-Aldrich</td>
			<td style="width:109px;">CLS7095D5X SIGMA</td>
			<td style="width:165px;">5.75 in length</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">hibernate-E Medium</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">A1247601</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">Pierce 16% formaldehyde</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">28906</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">PBS (10x)</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">QVC0508</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">normal goat serum</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">16210064</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">triton X-100</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;">28314</td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">anti-vGlut1 antibody</td>
			<td style="width:175px;">NeuroMab</td>
			<td style="width:109px;">75-066</td>
			<td style="width:165px;">clone N28/9, 1:100</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">anti-vGAT antibody</td>
			<td style="width:175px;">Synaptic Systems</td>
			<td style="width:109px;">131 003</td>
			<td style="width:165px;">1:1000</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:203px;">anti_beta-tubulin III</td>
			<td style="width:175px;">Aves</td>
			<td style="width:109px;">TUJ</td>
			<td style="width:165px;">1:1000</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">Alexa Fluor secondary antibodies</td>
			<td style="width:175px;">ThermoFisher Scientific</td>
			<td style="width:109px;"></td>
			<td style="width:165px;">1:1000</td>
		</tr>
		<tr height="25">
			<td height="25" style="height:25px;width:203px;">Incubator, 5% CO2 37 &#176;C</td>
			<td style="width:175px;"></td>
			<td style="width:109px;"></td>
			<td style="width:165px;"></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">Epifluorescence imaging system</td>
			<td style="width:175px;">EVOS Fluorescence imaging system</td>
			<td style="width:109px;">AMF4300</td>
			<td style="width:165px;">10x objective</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">Spinning disk confocal imaging system</td>
			<td style="width:175px;">Andor Technology</td>
			<td style="width:109px;">CSU-X1, iXon X3 EMCCD</td>
			<td style="width:165px;">60x silicone oil &#38; 20x objectives</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:203px;">Laser scanning confocal imaging system</td>
			<td style="width:175px;">Olympus</td>
			<td style="width:109px;">FV3000RS</td>
			<td style="width:165px;">30x silicone oil objective</td>
		</tr>
	</tbody>
</table>

use of pre-assembled plastic microfluidic chips for compartmentalizing primary murine neurons

Microfabricated methods to compartmentalize neurons have become essential tools for many neuroscientists. This protocol describes the use of a commercially available pre-assembled plastic chip for compartmentalizing cultured primary rat hippocampal neurons. These plastic chips, contained within the footprint of a standard microscope slide, are compatible with high-resolution, live, and fluorescence imaging. This protocol demonstrates how to retrograde label neurons via isolated axons using a modified rabies virus encoding a fluorescent protein, create isolated microenvironments within one compartment, and perform axotomy and immunocytochemistry on-chip. Neurons are cultured for &gt;3 weeks within the plastic chips, illustrating the compatibility of these chips for long-term neuronal cultures.

After approximately 5-7 days of neuron growth within the chip, axonal growth is evident. The chips are compatible with phase-contrast imaging as demonstrated in Figure 3, which shows neuronal growth at 24 days. The chips are also compatible with fluorescence imaging (Figure 4, Figure 5, Figure 6, and Figure&#160;7). Three days after rabies virus infection via the axonal compartment, mCherry-positive neurons with axons extending into the axonal compartment were imaged in the chip (Figure 4). To demonstrate the ability to fluidically isolate the compartments, a low molecular weight fluorescent dye (Alexa Fluor 488 hydrazide) was added to the axonal compartment. These results are comparable to PDMS-based chamber17 and demonstrate the suitability of the plastic chip for phase-contrast and fluorescence imaging.
To illustrate neuronal growth with the plastic chips and PDMS devices, we cultured neurons in both platforms and monitored neuronal growth over time. Figure 5 shows neuronal growth from 3 to 22 days in culture; these results are representative of 3 independent experiments. Neuronal growth is comparable within the two platforms up to 15 days in culture, but at longer culture ages (&#62;21 days) isolated axons within the plastic chip appear healthier with less beading (Figure 5A). To further visualize axons within the axonal compartments, we immunostained for &#946;-tubulin III which shows healthy axonal growth within the plastic chips at 22 days in culture (Figure 5B).
Axon injury and regeneration studies are common using microfluidic compartmentalized devices. To demonstrate the suitability of these studies using the chips, retrograde labeled neurons were imaged before and 24 h after axotomy (Figure 6). A retraction bulb and regenerating axon are both evident following axotomy. These results are equivalent to published data using PDMS-based devices14,17.
Immunocytochemistry is a common technique performed within multi-compartment devices to visualize protein localization. After 24 days in culture, neurons within the chips were fixed and stained for both excitatory and inhibitory synaptic markers, vGlut1 and vGat, respectively (Figure 7). Retrograde labeled mCherry neurons were also imaged (Figure 7C). Imaging was performed using spinning disk confocal with a 60&#215; silicone oil immersion objective, demonstrating the ability to perform high-resolution imaging. Importantly, dendritic spines were evident within a magnified region, demonstrating that the neurons cultured within the chips were forming mature synapses.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/58421/58421fig1.jpg" /> 
Figure 1: A pre-assembled, plastic two-compartment microfluidic chip for compartmentalizing neurons. (A) Schematic representation of the multicompartment chip showing the locations of the upper and lower wells. (B) An enlarged schematic of the chip showing the main channels (or compartments) and microgrooves which connect the compartments. The main channels are approximately 1.5 mm &#215; 7 &#215; 0.060 mm (W &#215; L &#215; H). The width and height of the microgrooves are approximately 0.01 mm &#215; 0.005 mm, respectively. The length of the microgrooves varies depending on the configuration, 0.15 mm to 0.9 mm. (C) A photograph of a representative multicompartment chip containing food coloring dye in each main channel or compartment demonstrating the ability to fluidically isolate each channel. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58421/58421fig1large.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/58421/58421fig2.jpg" /> 
Figure 2: Pipetting techniques needed when using plastic multicompartment chips. (A) When adding and aspirating media for washes, the pipet tip should be angled away from the entrance of the main channel as shown. (B) When loading neurons or performing axotomy, the pipet tip should be angled towards the entrance of the main channel. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58421/58421fig2large.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/58421/58421fig3.jpg" /> 
Figure 3: A phase contrast micrograph showing typical neuronal growth within the chip at 24 days in culture. Embryonic hippocampal neurons were seeded into the right somatic compartment. Axon growth is visible in the axonal compartment beginning at 5-7 days. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58421/58421fig3large.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/58421/58421fig4.jpg" /> 
Figure 4: Retrograde labeled neurons express mCherry fluorescent protein and extend axons into a fluidically isolated axonal compartment. (A) A merged fluorescence micrograph showing live retrograde labeled neurons infected via a modified mCherry rabies virus briefly applied to the axonal compartment. Neurons were imaged 3 days post-infection at 21 days in culture. Creating an isolated microenvironment within the axonal compartment is demonstrated by application of a low molecular weight dye, Alexa Fluor 488 hydrazide. (B) A merged image of (A) including a differential interference contrast (DIC) image to visualize the microgrooves region of the chip. Images were acquired with laser scanning confocal microscope using a 30&#215;/1.05 N.A. silicone oil (ne = 1.406) objective lens. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58421/58421fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/58421/58421fig5.jpg" /> 
Figure 5: Side-by-side comparison of neuronal growth within multicompartment PDMS devices and plastic chips. (A) Phase contrast micrographs of both platforms taken at 3, 7, 15, and 22 days in culture. At the bottom, a higher magnification region taken from the images at 22 days is included to illustrate axonal growth at this age within both platforms. Axons within the chip are more continuous and appear healthier than in the PDMS device at this age. (B) An invert immunofluorescence micrograph of &#946;-tubulin III stained axons within the axonal compartment of both the PDMS device and plastic chip at 22 days in culture. Images were acquired with a spinning disk confocal imaging system using a 20x/0.45 N.A. objective lens. All scale bars are 100 &#181;m. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58421/58421fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/58421/58421fig6.jpg" /> 
Figure 6: Axotomy and regeneration of hippocampal neurons within the plastic multicompartment chip. (Top) Neurons were retrograde labeled using a modified mCherry rabies virus and then imaged before axotomy at 24 days in culture. Images were pseudocolored using the &#39;Fire&#39; color look-up table. (Bottom) The same neuron imaged in the top panel was imaged 24 h post-axotomy. White dashed lines show the edges of the microgroove barrier. Axotomy occurred at the location of the left dashed line. The white arrowhead shows a retraction bulb. The white arrow indicates a regenerating axon. Images were acquired with a spinning disk confocal imaging system using a 20&#215;/0.45 N.A. objective lens. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58421/58421fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 7" class="xfigimg" src="/files/ftp_upload/58421/58421fig7.jpg" /> 
Figure 7: Synapses form between hippocampal neurons cultured within plastic multicompartment chips. Immunostaining was performed at 24 days in culture and imaged within the somatic compartment using a 60&#215; silicone oil immersion lens. Neurons express (A) the excitatory synapse marker, vGlut1 (green) and (B) the inhibitory synapse marker, vGAT (blue). (C) Retrograde labeled mCherry neurons (red) were infected via modified rabies virus applied to the axonal compartment. (D) A merged fluorescence micrograph of vGlut1, vGat, and mCherry. (E) The magnified region in (D) indicated with a white box shows dendritic spines, the sites that receive synaptic input from other neurons. Images were acquired with a spinning disk confocal imaging system using a 60&#215;/1.3 N.A. silicone oil (ne = 1.406) objective lens. <a href="https://jove.unicartagenaproxy.elogim.com/files/ftp_upload/58421/58421fig7large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Plastic multicompartment chips</td>
			<td>PDMS multicompartment devices</td>
		</tr>
		<tr>
			<td>isolate axons</td>
			<td>isolate axons</td>
		</tr>
		<tr>
			<td>establish microenvironments</td>
			<td>establish microenvironments</td>
		</tr>
		<tr>
			<td>axotomize neurons</td>
			<td>axotomize neurons</td>
		</tr>
		<tr>
			<td>optically transparent</td>
			<td>optically transparent</td>
		</tr>
		<tr>
			<td>compatible with high resolution imaging</td>
			<td>compatible with high resolution imaging</td>
		</tr>
		<tr>
			<td>compatible with fluorescence microscopy</td>
			<td>compatible with fluorescence microscopy</td>
		</tr>
		<tr>
			<td>fully assembled</td>
			<td>assembly to substrate required</td>
		</tr>
		<tr>
			<td>healthy axons &#62;21 days</td>
			<td>healthy axons &#62;14 days</td>
		</tr>
		<tr>
			<td>hydrophilic culturing surface</td>
			<td>hydrophobic</td>
		</tr>
		<tr>
			<td>gas impermeable</td>
			<td>gas permeable</td>
		</tr>
		<tr>
			<td>rounded microgrooves and channels</td>
			<td>straight microgrooves</td>
		</tr>
		<tr>
			<td>fewer preparation steps</td>
			<td>top is removable for staining within microgrooves</td>
		</tr>
		<tr>
			<td>not compatible with laser ablation</td>
			<td>absorption of small molecules &#38; organic solvents</td>
		</tr>
		<tr>
			<td>not compatible with mineral oil-based immersion oils (silicone-based oils are fine)</td>
			<td></td>
		</tr>
	</tbody>
</table>
Table 1:&#160;Comparison of plastic and PDMS multicompartment platforms for culturing neurons.

Watch this Scientific Journal Video about Use of Pre-Assembled Plastic Microfluidic Chips for Compartmentalizing Primary Murine Neurons at JoVE.com

Use of Pre-Assembled Plastic Microfluidic Chips for Compartmentalizing Primary Murine Neurons

This protocol describes the use of plastic chips to culture and compartmentalize primary murine neurons. These chips are preassembled, user-friendly, and compatible with high-resolution, live, and fluorescence imaging. This protocol describes how to plate rat hippocampal neurons within these chips and perform fluidic isolation, axotomy and immunostaining.

Microfabricated methods to compartmentalize neurons have become essential tools for many neuroscientists. This protocol describes the use of a ...

use-pre-assembled-plastic-microfluidic-chips-for-compartmentalizing

Loyola University Maryland

Research

JoVE Journal

Neuroscience

50.8K Views.  UNC Neuroscience Center. This protocol describes the use of plastic chips to culture and compartmentalize primary murine neurons. These chips are preassembled, user-friendly, and compatible with high-resolution, live, and fluorescence imaging. This protocol describes how to plate rat hippocampal neurons within these chips and perform fluidic isolation, axotomy and immunostaining. 

Video: Use of Pre-Assembled Plastic Microfluidic Chips for Compartmentalizing Primary Murine Neurons

Culturing and Electrophysiology of Cells on NRCC Patch-clamp Chips

Due to its exquisite sensitivity and the ability to monitor and control individual cells at the level of ion channels, patch-clamping is the gold standard of electrophysiology applied to disease models and pharmaceutical screens alike 1. The method traditionally involves gently contacting a cell with a glass pipette filled by a physiological solution in order to isolate a patch of the membrane under its apex 2. An electrode inserted in the pipette captures ion-channel activity within the membrane patch or, when ruptured, for the whole cell. In the last decade, patch-clamp chips have been proposed as an alternative 3, 4: a suspended film separates the physiological medium from the culture medium, and an aperture microfabricated in the film replaces the apex of the pipette. Patch-clamp chips have been integrated in automated systems and commercialized for high-throughput screening 5. To increase throughput, they include the fluidic delivery of cells from suspension, their positioning on the aperture by suction, and automated routines to detect cell-to-probe seals and enter into whole cell mode. We have reported on the fabrication of a silicon patch-clamp chip with optimized impedance and orifice shape that permits the high-quality recording of action potentials in cultured snail neurons 6; recently, we have also reported progress towards interrogating mammalian neurons 7. Our patch-clamp chips are fabricated at the Canadian Photonics Fabrication Centre 8, a commercial foundry, and are available in large series. We are eager to engage in collaborations with electrophysiologists to validate the use of the NRCC technology in different models. The chips are used according to the general scheme represented in Figure 1: the silicon chip is at the bottom of a Plexiglas culture vial and the back of the aperture is connected to a subterranean channel fitted with tubes at either end of the package. Cells are cultured in the vial and the cell on top of the probe is monitored by a measuring electrode inserted in the channel.The two outside fluidic ports facilitate solution exchange with minimal disturbance to the cell; this is an advantage compared to glass pipettes for intracellular perfusion.
<img alt="Figure 1" src="/files/ftp_upload/3288/3288fig1.jpg" />
Figure 1. Principle of measurement using the NRCC patch-clamp chip
We detail here the protocols to sterilize and prime the chips, load them with medium, plate them with cells, and finally use them for electrophysiological recordings.

We show how planar patch-clamp chips fabricated at the National Research Council of Canada are sterilized, primed, loaded with medium, plated with cells, and used for electrophysiological recordings.

Due to its exquisite sensitivity and the ability to monitor and control individual cells at the level of ion channels, patch-clamping is the gold standard ...

Calcium Phosphate Transfection of Primary Hippocampal Neurons

Calcium phosphate precipitation is a convenient and economical method for transfection of cultured cells. With optimization, it is possible to use this method on hard-to-transfect cells like primary neurons. Here we describe our detailed protocol for calcium phosphate transfection of hippocampal neurons cocultured with astroglial cells.

Calcium phosphate precipitation is a convenient and economical method for transfection of cultured cells. With optimization, it is possible to use this ...

Imaging Dendritic Spines of Rat Primary Hippocampal Neurons using Structured Illumination Microscopy

Dendritic spines are protrusions emerging from the dendrite of a neuron and represent the primary postsynaptic targets of excitatory inputs in the brain. Technological advances have identified these structures as key elements in neuron connectivity and synaptic plasticity. The quantitative analysis of spine morphology using light microscopy remains an essential problem due to technical limitations associated with light's intrinsic refraction limit. Dendritic spines can be readily identified by confocal laser-scanning fluorescence microscopy. However, measuring subtle changes in the shape and size of spines is difficult because spine dimensions other than length are usually smaller than conventional optical resolution fixed by light microscopy's theoretical resolution limit of 200 nm.
Several recently developed super resolution techniques have been used to image cellular structures smaller than the 200 nm, including dendritic spines. These techniques are based on classical far-field operations and therefore allow the use of existing sample preparation methods and to image beyond the surface of a specimen. Described here is a working protocol to apply super resolution structured illumination microscopy (SIM) to the imaging of dendritic spines in primary hippocampal neuron cultures. Possible applications of SIM overlap with those of confocal microscopy. However, the two techniques present different applicability. SIM offers higher effective lateral resolution, while confocal microscopy, due to the usage of a physical pinhole, achieves resolution improvement at the expense of removal of out of focus light. In this protocol, primary neurons are cultured on glass coverslips using a standard protocol, transfected with DNA plasmids encoding fluorescent proteins and imaged using SIM. The whole protocol described herein takes approximately 2 weeks, because dendritic spines are imaged after 16-17 days in vitro, when dendritic development is optimal. After completion of the protocol, dendritic spines can be reconstructed in 3D from series of SIM image stacks using specialized software.

This article describes a working protocol to image dendritic spines from hippocampal neurons in vitro using Structured Illumination Microscopy (SIM). Super-resolution microscopy using SIM provides image resolution significantly beyond the light diffraction limit in all three spatial dimensions, allowing the imaging of individual dendritic spines with improved detail.

Dendritic spines are protrusions emerging from the dendrite of a neuron and represent the primary postsynaptic targets of excitatory inputs in the brain. ...

Primary Culture of Mouse Dopaminergic Neurons

Dopaminergic neurons represent less than 1% of the total number of neurons in the brain. This low amount of neurons regulates important brain functions such as motor control, motivation, and working memory. Nigrostriatal dopaminergic neurons selectively degenerate in Parkinson&#39;s disease (PD). This progressive neuronal loss is unequivocally associated with the motors symptoms of the pathology (bradykinesia, resting tremor, and muscular rigidity). The main agent responsible of dopaminergic neuron degeneration is still unknown. However, these neurons appear to be extremely vulnerable in diverse conditions. Primary cultures constitute one of the most relevant models to investigate properties and characteristics of dopaminergic neurons. These cultures can be submitted to various stress agents that mimic PD pathology and to neuroprotective compounds in order to stop or slow down neuronal degeneration. The numerous transgenic mouse models of PD that have been generated during the last decade further increased the interest of researchers for dopaminergic neuron cultures. Here, the video protocol focuses on the delicate dissection of embryonic mouse brains. Precise excision of ventral mesencephalon is crucial to obtain neuronal cultures sufficiently rich in dopaminergic cells to allow subsequent studies. This protocol can be realized with embryonic transgenic mice and is suitable for immunofluorescence staining, quantitative PCR, second messenger quantification, or neuronal death/survival assessment.

Dopaminergic neurons play a vital regulatory role in the brain. Their loss is associated with Parkinson's disease. In this video, we show how to generate primary cultures of central dopaminergic neurons from embryonic mouse mesencephalon. Such cultures are useful to study the extreme vulnerability of these neurons to various stresses.

Dopaminergic neurons represent less than 1% of the total number of neurons in the brain. This low amount of neurons regulates important brain functions ...

Isolation of Primary Murine Brain Microvascular Endothelial Cells

The blood-brain-barrier is ultrastructurally assembled by a monolayer of brain microvascular endothelial cells (BMEC) interconnected by a junctional complex of tight and adherens junctions. Together with other cell-types such as astrocytes or pericytes, they form the neurovascular unit (NVU), which specifically regulates the interchange of fluids, molecules and cells between the peripheral blood and the CNS. Through this complex and dynamic system BMECs are involved in various processes maintaining the homeostasis of the CNS. A dysfunction of the BBB is observed as an essential step in the pathogenesis of many severe CNS diseases. However, specific and targeted therapies are very limited, as the underlying mechanisms are still far from being understood. 
Animal and in vitro models have been extensively used to gain in-depth understanding of complex physiological and pathophysiological processes. By reduction and simplification it is possible to focus the investigation on the subject of interest and to exclude a variety of confounding factors. However, comparability and transferability are also reduced in model systems, which have to be taken into account for evaluation. The most common animal models are based on mice, among other reasons, mainly due to the constantly increasing possibilities of methodology. In vitro studies of isolated murine BMECs might enable an in-depth analysis of their properties and of the blood-brain-barrier under physiological and pathophysiological conditions. Further insights into the complex mechanisms at the BBB potentially provide the basis for new therapeutic strategies.
This protocol describes a method to isolate primary murine microvascular endothelial cells by a sequence of physical and chemical purification steps. Special considerations for purity and cultivation of MBMECs as well as quality control, potential applications and limitations are discussed.

Brain microvascular endothelial cells (BMEC) are interconnected by specific junctional proteins forming a highly regulated barrier separating blood and the central nervous system (CNS), the so-called blood-brain-barrier (BBB). The isolation of primary murine brain microvascular endothelial cells, as discussed in this protocol, enables detailed in vitro studies of the BBB.

The blood-brain-barrier is ultrastructurally assembled by a monolayer of brain microvascular endothelial cells (BMEC) interconnected by a junctional ...

Modeling Neuronal Death and Degeneration in Mouse Primary Cerebellar Granule Neurons

Cerebellar granule neurons (CGNs) are a commonly used neuronal model, forming an abundant homogeneous population in the cerebellum. In light of their post-natal development, abundance, and accessibility, CGNs are an ideal model to study neuronal processes, including neuronal development, neuronal migration, and physiological neuronal activity stimulation. In addition, CGN cultures provide an excellent model for studying different modes of cell death including excitotoxicity and apoptosis. Within a week in culture, CGNs express N-methyl-D-aspartate (NMDA) receptors, a specific ionotropic glutamate receptor with many critical functions in neuronal health and disease. The addition of low concentrations of NMDA in conjunction with membrane depolarization to rodent primary CGN cultures has been used to model physiological neuronal activity stimulation while the addition of high concentrations of NMDA can be employed to model excitotoxic neuronal injury. Here, a method of isolation and culturing of CGNs from 6 day old pups as well as genetic manipulation of CGNs by adenoviruses and lentiviruses are described. We also present optimized protocols on how to stimulate NMDA-induced excitotoxicity, low-potassium-induced apoptosis, oxidative stress and DNA damage following transduction of these neurons.

This protocol describes a simple method for isolating and culturing primary mouse cerebral granule neurons (CGNs) from 6-7 day old pups, efficient transduction of CGNs for loss and gain of function studies, and modelling NMDA-induced neuronal excitotoxicity, low-potassium-induced cell death, DNA-damage, and oxidative stress using the same culture model.

Cerebellar granule neurons (CGNs) are a commonly used neuronal model, forming an abundant homogeneous population in the cerebellum. In light of their ...

High-resolution Volume Imaging of Neurons by the Use of Fluorescence eXclusion Method and Dedicated Microfluidic Devices

Volume is an important parameter regarding physiological and pathological characteristics of neurons at different time scales. Neurons are quite unique cells regarding their extended ramified morphologies and consequently raise several methodological challenges for volume measurement. In the particular case of in vitro neuronal growth, the chosen methodology should include sub-micrometric axial resolution combined with full-field observation on time scales from minutes to hours or days. Unlike other methods like cell shape reconstruction using confocal imaging, electrically-based measurements or Atomic Force Microscopy, the recently developed Fluorescence eXclusion method (FXm) has the potential to fulfill these challenges. However, although being simple in its principle, implementation of a high-resolution FXm for neurons requires multiple adjustments and a dedicated methodology. We present here a method based on the combination of fluorescence exclusion, low-roughness multi-compartments microfluidic devices, and finally micropatterning to achieve in vitro measurements of local neuronal volume. The high resolution provided by the device allowed us to measure the local volume of neuronal processes (neurites) and the volume of some specific structures involved in neuronal growth, such as growth cones (GCs).

Volume is an important parameter regarding physiological and pathological characteristics of cells. We describe a fluorescent exclusion method allowing full-field measurement of in vitro neuronal volume with sub-micrometric axial resolution required for the analysis of neurites and dynamic structures implied in neuronal growth.

Volume is an important parameter regarding physiological and pathological characteristics of neurons at different time scales. Neurons are quite unique ...

Isolation of Primary Murine Skeletal Muscle Microvascular Endothelial Cells

The endothelial cells of skeletal muscle capillaries (muscle microvascular endothelial cells, MMEC) build up the barrier between blood stream and skeletal muscles regulating the exchange of fluids and nutrients as well as the immune response against infectious agents by controlling immune cell migration. For these functions, MMEC form a functional &#34;myovascular unit&#34; (MVU), with further cell types, such as fibroblasts, pericytes and skeletal muscle cells. Consequently, a dysfunction of MMEC and therefore the MVU contributes to a vast variety of myopathies. However, regulatory mechanisms of MMEC in health and disease remain insufficiently understood and their elucidation precedes more specific treatments for myopathies. The isolation and in-depth investigation of primary MMEC functions in the context of the MVU might facilitate a better understanding of these processes.
This article provides a protocol to isolate primary murine MMEC of the skeletal muscle by mechanical and enzymatic dissociation including purification and culture maintenance steps.

Microvascular endothelial cells of skeletal muscles (MMEC) shape the inner wall of muscle capillaries and regulate both, exchange of fluids/molecules and migration of (immune) cells between muscle tissue and blood. Isolation of primary murine MMEC, as described here, enables comprehensive in vitro investigations of the &#34;myovascular unit&#34;.

The endothelial cells of skeletal muscle capillaries (muscle microvascular endothelial cells, MMEC) build up the barrier between blood stream and skeletal ...

Compartmentalization of Human Stem Cell-Derived Neurons within Pre-Assembled Plastic Microfluidic Chips

Use of microfluidic devices to compartmentalize cultured neurons has become a standard method in neuroscience. This protocol shows how to use a pre-assembled multi-compartment chip made in a cyclic olefin copolymer (COC) to compartmentalize neurons differentiated from human stem cells. The footprint of these COC chips are the same as a standard microscope slide and are equally compatible with high resolution microscopy. Neurons are differentiated from human neural stem cells (NSCs) into glutamatergic neurons within the chip and maintained for 5 weeks, allowing sufficient time for these neurons to develop synapses and dendritic spines. Further, we demonstrate multiple common experimental procedures using these multi-compartment chips, including viral labeling, establishing microenvironments, axotomy, and immunocytochemistry.

This protocol demonstrates the use of compartmentalized microfluidic chips, injection molded in a cyclic olefin copolymer to cultured neurons differentiated from human stem cells. These chips are preassembled and easier-to-use than traditional compartmentalized poly(dimethylsiloxane) devices. Multiple common experimental paradigms are described here, including viral labeling, fluidic isolation, axotomy, and immunostaining.

Use of microfluidic devices to compartmentalize cultured neurons has become a standard method in neuroscience. This protocol shows how to use a ...

Primary Culture of Neurons Isolated from Embryonic Mouse Cerebellum

The use of primary cell cultures has become one of the major tools to study the nervous system in vitro. The ultimate goal of using this simplified model system is to provide a controlled microenvironment and maintain the high survival rate and the natural features of dissociated neuronal and nonneuronal cells as much as possible under in vitro conditions. In this article, we demonstrate a method of isolating primary neurons from the developing mouse cerebellum, placing them in an in vitro environment, establishing their growth, and monitoring their viability and differentiation for several weeks. This method is applicable to embryonic neurons dissociated from cerebellum between embryonic days 12&ndash;18.

Conducting in vitro experiments to reflect in vivo conditions as adequately as possible is not an easy task. The use of primary cell cultures is an important step toward understanding cell biology in a whole organism. The provided protocol outlines how to successfully grow and culture embryonic mouse cerebellar neurons.

The use of primary cell cultures has become one of the major tools to study the nervous system in vitro. The ultimate goal of using this simplified model ...