The authors would like to thank Hartwig Wieboldt for his excellent technical assistance, and the UKE Microscopy Imaging Facility (Umif) of the University Medical Center Hamburg-Eppendorf for providing microscopes and support. This research was funded by the DZHK (German Centre for Cardiovascular Research) [FKZ 81Z4710141].

All procedures involving animals were approved by the Animal Care and Use Committee of the State of Hamburg (ORG870, 959) and the North Rhine-Westphalian State Agency for Nature, Environment and Consumer Protection (LANUV, 07/11) and conform to the National Institutes of Health&#39;s Guide for the Care and Use of Laboratory Animals (2011). Studies were performed using male and female (aged 10-24 weeks) C57BL/6 mice (stock number 000664, Jackson Laboratories) and mice homozygous (db/db) or heterozygous (db/het; control) for the diabetes spontaneous mutation (Leprdb; BKS.Cg-Dock7m+/+ Leprdb&#160;/J, stock number 000642, Jackson Laboratories). The authors have used the protocols at hand without variations for mice aged up to 60 weeks.
1. Location and dissection of murine stellate ganglia
NOTE: Even though descriptions and drawings are mostly available in bigger species, some publications have previously described the location of the SG in rats24 and mice25 using anatomical methods and fluorescent reporter lines, respectively.
<ol>
	<li>Prepare 50 mL of ice-cold (3-4 &#176;C) heparinized (20&#160;units/mL, see Table of Materials) phosphate-buffered saline (PBS). Perform dissection of the SG at room temperature (RT).</li>
	<li>Deeply anesthetize mouse by inhalation of 3%-5% isoflurane according to the institutional and local guidelines. Verify adequate anesthesia by loss of pedal withdrawal reflex. Decapitate mice or perform cervical dislocation. 
	NOTE: Incorrect cervical dislocation can result in breakage of the spine and damage of thoracic vessels leading to bleeding which hinders the preparation or&#160;severing of the sympathetic chain, so that SG are not in their correct position. Therefore, it is critical to have experienced personnel perform cervical dislocation or decapitate animals in deep sedation.</li>
	<li>Spray the skin with ethanol and open the thorax with two incisions along the anterior axillary lines using Mayo scissors and narrow pattern forceps. Cut the diaphragm and remove the front of the&#160;ribcage.</li>
	<li>Remove the heart-lung package by gripping the aorta and vena cava right above the diaphragm using London forceps and cutting all vessels and connective tissue close to the spine below with the Strabismus scissors.</li>
	<li>Flush the thorax thoroughly with heparinized PBS using a plastic disposable pipette until all traces of blood are removed.</li>
	<li>Place the torso under stereomicroscope preparation binoculars and ensure good lighting in the thorax with external light sources.</li>
	<li>Locate the first rib and the longus colli muscles. 
	NOTE: The SG are located bilaterally, parallel to the spine at the branch between the first rib and the spine, in a groove lateral to the longus colli muscles24. The flat side of the SG is located adjacent to the longus colli muscles. Depending on the preparation, parts of the sympathetic chain might already be visible as white, oblique fibers parallel to the spine. These can be traced along to the SG.</li>
	<li>Gently use the tip of the Dumont #5/45 forceps to expose the connective tissue lateral to the longus colli muscle.</li>
	<li>Turn the forceps around by 180&#176; and use the flat side to grip the SG and pull it out with minimal pressure.</li>
	<li>Repeat with the second SG.</li>
	<li>Place both SG in a dish (6 cm diameter) filled with cold PBS and inspect with the appropriate magnification. If necessary, remove excess vessels, fat tissue, and larger nerves. 
	NOTE: Autonomic ganglia are surrounded by a connective tissue capsule consisting of collagen fibers and fibroblasts26,27.The permeability of these capsules seems to vary among species, different kind of ganglia26 and age28. Remove as much connective tissue as possible using Dumont #5/45 forceps and, if necessary, spring scissors.</li>
	<li>Depending on the goal of the experiment, proceed with section 2, 3, or 5&#160;of this protocol.</li>
</ol>
2. Whole mount immunohistochemistry protocol
NOTE: This protocol is adapted from cardiac whole mount stainings4,29. Perform incubation steps for every single SG in one well of a 96-well plate and use 100 &#956;L (for antibody-containing solutions) to 200 &#956;L (for all other solutions) of the solution to ensure complete coverage. Regularly check the coverage and correct immersion of the SG with binoculars. Remove liquids manually with a 200 &#956;L pipette with an additional 10 &#956;L tip on top of the 200 &#956;L tip. This will prevent aspiration of the SG in the pipette tip. Use freshly prepared solutions and sterile liquids to prevent bacterial growth.
<ol>
	<li>Fix SG for histology for 2 h at RT in 4% methanol-free paraformaldehyde (PFA)/PBS.</li>
	<li>Process SG as quickly as possible, but they can be stored for 2-4 weeks at 4-6 &#176;C in PBS with 0.02% (w/v) sodium azide at this point.</li>
	<li>Prepare Sudan black stock solution (1% Sudan black w/v in 100% ethanol) for reduction of autofluorescence and improvement of signal to background ratio30. Dissolve for 2-3 h on a magnetic stirrer at RT. 
	NOTE: Use the stock solution for a maximum of 6-8 weeks, discard earlier when sedimentation appears.</li>
	<li>Prepare Sudan black working solution by centrifuging the stock solution for 30 min at full speed (13,000 x g) to remove debris and diluting the stock in 70% ethanol to a final concentration of 0.25% Sudan black.</li>
	<li>Treat SG with Dent&#39;s bleach to improve antibody permeabilization31. Freshly prepare Dent&#39;s bleach by mixing methanol (MeOH), hydrogen peroxide solution 30% (w/w) in H2O and dimethyl sulfoxide (DMSO) in a ratio of 4:1:1. Add 200 &#956;L per SG and place the plate on an orbital shaker for 1 h at RT.</li>
	<li>Perform a descending MeOH series for rehydration by incubating for 10 min each on an orbital shaker: 100% MeOH, 75% MeOH/PBS, 50% MeOH/PBS, 25% MeOH/PBS.</li>
	<li>Perform permeabilization by incubating SG twice for 60 min each in PBS/1% Triton-X-100 at RT.</li>
	<li>Remove permeabilization solution from the SG and add Sudan black working solution. Incubate for 2 h at RT on an orbital shaker.</li>
	<li>In the meantime, prepare a blocking solution by adding 5% receptor grade bovine serum albumin (BSA) and 0.1% Triton-X-100 in PBS a 15 mL vessel and let it dissolve on a roller shaker for approximately 5-10 min. Decant through a pre-pleated paper filter to remove debris.</li>
	<li>Remove Sudan black very carefully by tilting the plate and carefully pipetting from the upright side. 
	NOTE: It is not possible to see the SG in Sudan black. Use a strong light source and work slowly. From this step on, SG are stained black, enhancing visibility. If any additional connective tissue is seen surrounding SG at this point, remove it using Dumont #5/45 forceps and spring scissors.</li>
	<li>Add 200 &#956;L of PBS/0.1% Triton-X-100 (PBS-T) and wash for 5 min at RT on an orbital shaker.</li>
	<li>Remove PBS-T by aspirating it with a pipette and repeat 2 times.</li>
	<li>Remove PBS; add 200 &#956;L of blocking solution and incubate at 4 &#176;C overnight on an orbital shaker.</li>
	<li>On the next day, prepare solutions by adding primary antibodies in the blocking solution. Adapt antibody concentrations from established protocols. 
	NOTE: Include one SG as antibody control without primary antibody (incubated with antigen-preabsorbed antibody or IgG, if available, or blocking buffer).</li>
	<li>Perform primary antibody incubation for 36-48 h at 4 &#176;C on an orbital shaker. For cell size measurements and staining of sympathetic neurons, use antibodies against tyrosine hydroxylase (see Table of Materials for antibody recommendations). 
	NOTE: Place the 96-well plate in a wet chamber (e.g., plastic box lined with ddH2O-wetted paper towels) to prevent evaporation at this point.</li>
	<li>Remove antibody solution carefully and add 200 &#956;L of PBS-T. Place the plate on an orbital shaker for 30 min.</li>
	<li>Remove PBS-T and repeat the washing step 5 additional times.</li>
	<li>Prepare the secondary antibody working solution by centrifuging fluorescent Alexa-labeled secondary antibodies for 1 min at full speed (13,000 x g) before usage. Dilute the appropriate secondary antibodies according to the primary antibodies 1:500 in the blocking solution and add to SG. Add 1 &#956;g/mL of bisbenzimide H33342 trihydrochloride (Hoechst staining) if nuclear staining is desired. Incubate for 12-24 h at 4 &#176;C on an orbital shaker.</li>
	<li>Remove the antibody solution carefully and add 200 &#956;L of PBS-T. Place the plate on an orbital shaker for 30 min.</li>
	<li>Remove PBS-T and repeat the washing step 5 additional times. For the last step, use PBS without Triton.</li>
	<li>For embedding, spread 50-100 &#956;L of fluorescent mounting medium (see Table of Materials) on a glass slide and place under preparation binoculars. Use Dumont #5/45 forceps to pick up SG from the 96-well plate and remove excess liquid by dipping one end on a filter paper (e.g., Whatman drying pad) and place it on the drop.</li>
	<li>Use Dumont #5/45 forceps to correct positioning with the appropriate magnification.</li>
	<li>Gently place a glass coverslip (20 mm x 20 mm) next to the SG and slowly descend. 
	NOTE: Using too much mounting medium will result in movement of the SG or tangling of nerves. If that happens, quickly remove the coverslip and repeat steps 2.9-2.21.</li>
	<li>Let the slides dry in the dark overnight at RT. Storage of the stained specimen is possible for at least 4-6 weeks at 4 &#176;C.</li>
</ol>
3. Whole mount in situ hybridization
NOTE: Whole-mount in situ-hybridization of the SG is adapted from the organ of corti32 and the commercial RNA fluorescence in situ protocol (see Table of Materials). Obtain probes for the genes of interest and buffers and solutions from the supplier. All incubation steps are performed at RT, if not mentioned otherwise. Use sterile PBS. If interested in staining several SG in one well, use at least 150 &#956;L of buffers and solutions.
<ol>
	<li>Perform dissection of the SG as described in steps 1.1-1.13.</li>
	<li>Fixate SG for 1 h in 200 &#956;L of 4% MeOH-free PFA/PBS in one well of a 96-well plate placed on an orbital shaker.</li>
	<li>Wash SG three times for 30 min each in 0.1% Tween-20/PBS on an orbital shaker.</li>
	<li>Dehydrate SG in MeOH/PBS series by subsequent incubation in 50% MeOH/PBS, 70% MeOH/PBS, and 100% MeOH for 10 min each on an orbital shaker.</li>
	<li>Store SG at -20 &#176;C in 100% MeOH overnight.</li>
	<li>The next day, pre-warm the incubator to 40 &#176;C. Check the temperature with a thermometer.</li>
	<li>Rehydrate SG in reverse MeOH/PBS series (100% MeOH, 70% MeOH/PBS, 50% MeOH/PBS) for 10 min each.</li>
	<li>Wash SG three times for 5 min each in PBS.</li>
	<li>In the meantime, start pre-warming the probes by incubation at 40 &#176;C for 10 min, followed by cooling for 10 min.</li>
	<li>Incubate SG in 200 &#956;L of Protease III for 15 min.</li>
	<li>Optional: Perform Sudan black treatment to quench autofluorescence according to sections 2.3, 2.4, and 2.8 of this protocol if subsequent immunofluorescence staining is planned.</li>
	<li>Wash SG in 200 &#956;L of 0.1% Tween-20/PBS 3x for 5 min each on an orbital shaker.</li>
	<li>Optional: If co-staining with several probes is desired, dilute Channel-2 (50x) and Channel-3 probe (50x) in Channel-1 probe (1x).</li>
	<li>Cover SG with 100 &#956;L of probe for the gene of interest and incubate overnight at 40 &#176;C with slight agitation. Place the 96-well plate in a wet chamber at 40 &#176;C for all incubation steps. 
	NOTE: Include one SG as negative control, using a probe against a bacterial gene (e.g., dihydro-dipicolinate reductase, Dapb) to check for non-specific binding of amplification reagents in later steps.</li>
	<li>Wash SG in supplied washing buffer 3x for 15 min each on an orbital shaker.</li>
	<li>Pre-warm Amp1-3, HRP-C1, and HRP-Blocker to RT. If co-staining with Channel-2 and/or Channel-2 probe is desired, pre-warm HRP-C2 and HRP-C3.</li>
	<li>Re-fix SG for 10 min at RT in 4% PFA/PBS on an orbital shaker.</li>
	<li>Wash SG in 200 &#956;L of supplied washing buffer 3x for 5 min each on an orbital shaker at RT.</li>
	<li>For amplification, incubate SG with 100 &#956;L of Amp1 for 35 min at 40 &#176;C on an orbital shaker.</li>
	<li>Carefully remove any liquid and wash SG in 200 &#956;L of supplied washing buffer 3x for 5 min each at RT on an orbital shaker.</li>
	<li>Incubate SG with 100 &#956;L of Amp2 for 35 min at 40 &#176;C on an orbital shaker.</li>
	<li>Repeat step 3.18.</li>
	<li>Incubate SG with 100 &#956;L of Amp3 for 20 min at 40 &#176;C on an orbital shaker.</li>
	<li>Repeat step 3.18.</li>
	<li>Incubate SG with 100 &#956;L of supplied Multiplex FL v2 HRP-C1 for 20 min at 40 &#176;C on an orbital shaker.</li>
	<li>Repeat step 3.18.</li>
	<li>Prepare Opal-conjugated secondary antibody 1:1,000 in 200 &#956;L of supplied TSA-buffer and incubate SG for 35 min at 40 &#176;C on an orbital shaker. Protect from light during incubation and from this step on.</li>
	<li>Repeat step 3.18.</li>
	<li>Incubate SG in 100 &#956;L of supplied Multiplex FL v2 HRP-blocker for 15 min at 40 &#176;C on an orbital shaker.</li>
	<li>Repeat step 3.18.</li>
	<li>Optional: For co-staining with Channel-2 probe, repeat steps 3.25-3.30 with supplied Multiplex FL v2 HRP-C2.</li>
	<li>Optional: For co-staining with Channel-3 probe, repeat steps 3.25-3.30 with supplied Multiplex FL v2 HRP-C3.</li>
	<li>In case of subsequent immunofluorescent staining, perform steps 2.13-2.25 of this protocol.</li>
	<li>Incubate in 1% BSA/PBS for 30 min on an orbital shaker.</li>
	<li>Incubate SG for 30 min in 1 &#956;g/mL of bisbenzimide H33342 trihydrochloride (Hoechst staining) in 1% BSA/PBS if nuclear staining is desired and/or add Alexa-coupled wheat germ agglutinin (WGA, 1:500) on an orbital shaker.</li>
	<li>Repeat step 3.18.</li>
	<li>Embed as described in steps 2.19-2.22.</li>
</ol>
4. Imaging and analyses of murine stellate ganglia
<ol>
	<li>Perform confocal microscopy of embedded SG in the local imaging facility.</li>
	<li>If cell size measurements are required, image SG stained for tyrosine hydroxylase (see Table of Materials) at 200x magnification and take 4-6 random images from every SG.</li>
	<li>Analyze images using ImageJ33 software to estimate cell size (e.g., with a pen table, see Table of Materials). Use Free Hand Selection, circle each cell and click on Analyze | Measure to obtain cell area. Be careful to include only intact, fully visible cells that are located well within the SG.</li>
	<li>Using this method, perform measurement of approximately 100 cells per SG.</li>
	<li>Have a blinded investigator perform steps 4.2-4.3 if you want to compare SG from different mice. Use a frequency distribution in statistical software to visualize size differences between groups34.</li>
</ol>
5. Molecular analyses of murine stellate ganglia
NOTE: Include controls depending on your experimental design. This could be SG with different genotypes and disease background and/or other autonomic ganglia, such as the sympathetic superior cervical ganglion (located in the neck area, see detailed description in Ziegler et al.35) or parasympathetic ganglia (such as intracardiac ganglia, see Jungen et al.4).
<ol>
	<li>Prepare a 2 mL tube with 500 &#956;L of phenol/guanidine thiocyanate solution (e.g., Qiazol) per animal and have liquid nitrogen ready for shock-frosting or consider commercial solutions for protection of RNA (optional, see Table of Materials)36. Work quickly for RNA isolation.</li>
	<li>Perform dissection of the SG as described in steps 1.1-1.13.</li>
	<li>Immediately immerse both SG directly in one tube with phenol/guanidine thiocyanate solution and shock-frost tube in liquid nitrogen.</li>
	<li>Store at -80 &#176;C until further processing.</li>
	<li>For tissue lysis, let tubes with SG thaw until phenol/guanidine thiocyanate solution is liquified and add two 7 mm stainless steel beads. Cool down the metal parts of tissue homogenizer (ball or mixer mill, e.g., Tissue Lyser II) on dry ice and centrifuge at&#160;4 &#176;C.</li>
	<li>Centrifuge tubes at 500 x g for 1 min at 4 &#176;C so that SG are at the bottom of the tube.</li>
	<li>Put tubes into the metal parts of the Tissue Lyser and lyse for 1 min at 20 Hz.</li>
	<li>Repeat steps 5.6 and 5.7 up to 5 times until no intact tissue is detectable.</li>
	<li>Transfer the liquid into a fresh 1.5 mL tube.</li>
	<li>Perform RNA isolation with a column-based RNA isolation kit (e.g., miRNeasy mini kit) according to the manufacturer&#39;s instructions.</li>
	<li>Elute RNA in 20 &#956;L of RNase-free water and measure concentration using a spectrophotometer. 
	NOTE: To exclude contamination of the purified RNA with genomic DNA, we propose performing a polymerase chain reaction with genomic primers and 1 &#956;L of RNA as template, instead minus reverse transcriptase control. This will save a significant amount of RNA. If RNA is contaminated, use exon-intron boundary primers or intron flanking primers for subsequent quantitative real-time polymerase chain reaction.</li>
	<li>Use 250 ng SG RNA to perform cDNA synthesis and use established protocols. Here, a high-capacity cDNA reverse transcription kit was used according to the manufacturer&#39;s instructions.</li>
	<li>Dilute to a final concentration of 2.5 ng/&#956;L of cDNA and perform quantitative real-time polymerase chain reaction with the appropriate probes according to the established protocols. Here, TaqMan Assay (see Table of Materials) was performed using 10 ng cDNA per reaction. 
	NOTE: Perform no-template control for every gene to exclude false positive results.</li>
	<li>Normalize gene expression of your gene of interest on a house keeping gene (e.g., Cdkn1b) to compare relative gene expression between different groups of SG.</li>
</ol>

The authors have nothing to disclose.

The understanding of cellular and molecular processes in neurons and glial cells of the sympathetic nervous system that precede the onset of VA is of high interest, as sudden cardiac arrest remains the most common cause of death worldwide5. Therefore, in the current manuscript, we provide a basic repertoire of methods to identify the murine SG&#160;&#8211;&#160;a murine&#160;element within&#160;this network &#8211;&#160;and perform subsequent analyses on RNA, protein, and cellular level.
<p cl...

The cardiac autonomic nervous system is a tightly regulated equilibrium of sympathetic, parasympathetic, and sensory components that allows the heart to adapt to environmental changes with the appropriate physiological response1,2. Disturbances in this equilibrium, for example, an increase of sympathetic activity, have been established as a key driver for the onset as well as maintenance of ventricular arrhythmias (VA)3,4. Therefore, autonomic modulation, achieved via pharmacological reduction of sympathetic activity with beta-blockers, has been a cornerstone in the treatment of patients with VA for decades5,6. But despite pharmacological and catheter-based interventions, a relevant number of patients still suffers from recurrent VA7.
Sympathetic input to the heart is mostly mediated via neuronal cell bodies in the stellate ganglia (SG), bilateral star-shaped structures of the sympathetic chain, which relay information via numerous intrathoracic nerves from the brainstem to the heart8,9,10. Nerve sprouting from the SG after injury is associated with VA and sudden cardiac death11,12, emphasizing the SG as a target for autonomic modulation13,14. A reduction of sympathetic input to the heart can be achieved temporarily via percutaneous injection of local anesthetics or permanently by partial removal of the SG via video-assisted thoracoscopy15,16. Cardiac sympathetic denervation presents an option for patients with therapy-refractory VA with promising results14,16,17. We have learned from explanted SG of these patients that neuronal and neurochemical remodeling, neuro-inflammation and glial activation are hallmarks of sympathetic remodeling that might contribute or aggravate autonomic dysfunction18,19. Still, the underlying cellular and molecular processes in these neurons remain obscure to date, for example, the role of neuronal transdifferentiation into a cholinergic phenotype20,21. Experimental studies present novel approaches to treat VA, for example, the reduction of sympathetic nerve activity via optogenetics22, but in-depth characterization of the SG is still lacking in many cardiac pathologies that go in hand with VA. Mouse models mimicking these pathologies allow to study neuronal remodeling that potentially precedes the onset of arrhythmias12,23. These can be completed by further morphological and functional analyses for autonomic characterization of the heart and the nervous system. In the present protocol, we provide a basic repertoire of methods allowing to dissect and characterize the murine SG to improve the understanding of VA.

<table><tbody><tr><td>96-well plate</td><td>TPP</td><td>92097</td><td>RNAscope</td></tr><tr><td>Adhesion Slides SuperFrost plus&amp;nbsp; 25 x 75 x 1 mm</td><td>R. Langenbrinck</td><td>03-0060</td><td>Microscopy</td></tr><tr><td>Albumin bovine Fraction V receptor grade lyophil.</td><td>Serva</td><td>11924.03</td><td>Whole mount staining</td></tr><tr><td>bisBenzimide H33342 trihydrochloride (Hoechst)</td><td>Sigma-Aldrich, St. Louis, MO, USA</td><td>B2261</td><td>Whole mount staining</td></tr><tr><td>Chicken anti neurofilament</td><td>EMD Millipore</td><td>AB5539</td><td>Whole mount staining</td></tr><tr><td>Dimethyl sulfoxide (DMSO)</td><td>Merck, KGA, Darmstadt, Germany</td><td>D8418</td><td>Whole mount staining</td></tr><tr><td>Donkey anti chicken IgY Alexa 647&amp;nbsp;</td><td>Merck, KGA, Darmstadt, Germany</td><td>AP194SA6</td><td>Whole mount staining</td></tr><tr><td>Donkey anti goat IgG Alexa 568&amp;nbsp;</td><td>Thermo Fisher Scientific</td><td>A11057</td><td>Whole mount staining</td></tr><tr><td>Donkey anti rabbit IgG Alexa 488&amp;nbsp;</td><td>Thermo Fisher Scientific</td><td>A21206</td><td>Whole mount staining</td></tr><tr><td>Drying block 37-100 mm</td><td>Whatman (Sigma Aldrich)</td><td>WHA10310992&amp;nbsp;</td><td>Whole mount staining</td></tr><tr><td>Eosin Y</td><td>Sigma Aldrich</td><td>E4009</td><td>Whole mount staining</td></tr><tr><td>Ethanol 99 % denatured with MEK, IPA and Bitrex (min. 99,8 %)</td><td>Th.Geyer</td><td>2212.5000</td><td>Whole mount staining</td></tr><tr><td>Eukitt mounting medium</td><td>AppliChem</td><td>253681.0008</td><td>Whole mount staining</td></tr><tr><td>Fluoromount-G</td><td>Southern Biotech</td><td>0100-01</td><td>Whole mount staining</td></tr><tr><td>Fluoromount-G + DAPI</td><td>Southern Biotech</td><td>0100-20</td><td>Whole mount staining</td></tr><tr><td>Goat anti choline acetyltransferase</td><td>EMD Millipore</td><td>AP144P</td><td>Whole mount staining</td></tr><tr><td>H&lt;sub&gt;2&lt;/sub&gt;O&lt;sub&gt;2&lt;/sub&gt; 30% (w/w)</td><td>Merck, KGA, Darmstadt, Germany</td><td>H1009</td><td>Whole mount staining</td></tr><tr><td>Heparin Sodium 25.000 UI / 5ml</td><td>Rotexmedica</td><td>PZN: 3862340</td><td>Preparation SG</td></tr><tr><td>High-capacity cDNA reverse transctiption kit</td><td>Life technologies</td><td>&amp;nbsp;4368813</td><td>RNA isolation</td></tr><tr><td>Isoflurane (Forene)</td><td>Abbott Laboratories</td><td>2594.00.00</td><td>Preparation SG</td></tr><tr><td>Mayer&#039;s hemalum solution</td><td>Merck</td><td>1.09249.0500</td><td>Whole mount staining</td></tr><tr><td>Methanol</td><td>Sigma-Aldrich</td><td>34860</td><td>Whole mount staining</td></tr><tr><td>Microscope cover glasses 20x20 mm or smaller</td><td>Marienfeld</td><td>0101040</td><td>Whole mount staining</td></tr><tr><td>miRNeasy Mini Kit</td><td>Qiagen</td><td>217004</td><td>RNA isolation</td></tr><tr><td>NanoDrop 2000c</td><td>Thermo Fisher Scientific</td><td>ND-2000C</td><td>RNA isolation</td></tr><tr><td>Opal 570 Reagent Pack</td><td>Akoya Bioscience</td><td>FP1488001KT</td><td>RNAscope</td></tr><tr><td>Paraformaldehyde, 16% w/v aq. soln., methanol free&amp;nbsp;</td><td>Alfa Aesar</td><td>43368</td><td>Whole mount staining</td></tr><tr><td>Pasteur pipettes, LDPE, unsterile, 3 ml, 154 mm</td><td>Th.Geyer</td><td>7691202</td><td>Whole mount staining</td></tr><tr><td>Phosphate-buffered saline tablets</td><td>Gibco</td><td>18912-014</td><td>Whole mount staining</td></tr><tr><td>Pinzette Dumont SS Forceps</td><td>FineScienceTools</td><td>11203-25</td><td>Preparation SG</td></tr><tr><td>QIAzol Lysis Reagent</td><td>Qiagen&amp;nbsp;</td><td>79306</td><td>RNA isolation</td></tr><tr><td>Rabbit anti tyrosine hydroxylase</td><td>EMD Millipore</td><td>AB152</td><td>Whole mount staining</td></tr><tr><td>RNAlater</td><td>Merck</td><td>R0901-100ML</td><td>RNA isolation (optional)</td></tr><tr><td>RNAscope Multiplex Fluorescent Reagent Kit v2</td><td>biotechne (ACD)</td><td>323100</td><td>RNAscope</td></tr><tr><td>RNAscope Probe-Mm-S100b-C2</td><td>biotechne (ACD)</td><td>431738-C2</td><td>RNAscope</td></tr><tr><td>RNAscope Probe-Mm-Tubb3</td><td>biotechne (ACD)</td><td>423391</td><td>RNAscope</td></tr><tr><td>Stainless steel beads 7 mm&amp;nbsp;</td><td>Qiagen&amp;nbsp;</td><td>69990</td><td>RNA isolation</td></tr><tr><td>Sudan black B</td><td>Roth</td><td>0292.2</td><td>Whole mount staining</td></tr><tr><td>TaqMan Gene Expression Assay Cdkn1b (Mm00438168_m1)</td><td>Thermo Fisher Scientific</td><td>4331182</td><td>Gene expression analysis</td></tr><tr><td>TaqMan Gene Expression Assay Choline acetyltransferase (Mm01221880_m1)</td><td>Thermo Fisher Scientific</td><td>4331182</td><td>Gene expression analysis</td></tr><tr><td>TaqMan Gene Expression Assay MKi67 (Mm01278617_m1)</td><td>Thermo Fisher Scientific</td><td>4331182</td><td>Gene expression analysis</td></tr><tr><td>TaqMan Gene Expression Assay PTPCR (Mm01293577_m1)</td><td>Thermo Fisher Scientific</td><td>4331182</td><td>Gene expression analysis</td></tr><tr><td>TaqMan Gene Expression Assay S100b (Mm00485897_m1)</td><td>Thermo Fisher Scientific</td><td>4331182</td><td>Gene expression analysis</td></tr><tr><td>TaqMan Gene Expression Assay Tyrosin Hydroxylase (Mm00447557_m1)</td><td>Thermo Fisher Scientific</td><td>4331182</td><td>Gene expression analysis</td></tr><tr><td>TaqMan mastermix</td><td>Applied biosystems</td><td>4370074</td><td>Gene Expression analysis&amp;nbsp;</td></tr><tr><td>Tissue Lyser II</td><td>Qiagen</td><td>85300</td><td>RNA isolation</td></tr><tr><td>Triton X-100 10% solution</td><td>Sigma-Aldrich</td><td>93443-100ml</td><td>Whole mount staining</td></tr><tr><td>Tween-20</td><td>Sigma-Aldrich</td><td>P9416-100ML</td><td>RNAscope</td></tr><tr><td>Wacom bamboo pen</td><td>Wacom</td><td>CTL-460/K</td><td>Cell size measurements</td></tr><tr><td>Whatman prepleated qualitative filter paper, Grade 595 1/2</td><td>Sigma-Aldrich</td><td>WHA10311647</td><td>Whole mount staining</td></tr><tr><td>Wheat Germ Agglutinin, Alexa Fluor 633 Conjugate</td><td>Thermo Fisher Scientific</td><td>W21404</td><td>RNAscope</td></tr></tbody></table>

location, dissection, and analysis of the murine stellate ganglion

The autonomic nervous system is a substantial driver of cardiac electrophysiology. Especially&#160;the role of its sympathetic branch is an ongoing matter of investigation in the pathophysiology of ventricular arrhythmias (VA). Neurons in the stellate ganglia (SG)&#160;&#8211;&#160;bilateral star-shaped structures of the sympathetic chain &#8211;&#160;are an important component of the sympathetic infrastructure. The SG are a recognized target for&#160;treatment via cardiac sympathetic denervation in patients with therapy-refractory VA. While neuronal remodeling and glial activation in the SG have been described in patients with VA, the underlying cellular and molecular processes that potentially precede the onset of arrhythmia are only insufficiently understood and should be elucidated to improve autonomic modulation. Mouse models allow us to study sympathetic neuronal remodeling, but identification of the murine SG is challenging for the inexperienced investigator. Thus, in-depth cellular and molecular biological studies of the murine SG are lacking for many common cardiac diseases. Here, we describe a basic repertoire for dissecting and studying the SG in adult mice for analyses at RNA level (RNA isolation for gene expression analyses, in situ hybridization), protein level (immunofluorescent whole mount staining), and cellular level (basic morphology, cell size measurement). We present potential solutions to overcome challenges in the preparation technique, and how to improve staining via quenching of autofluorescence. This allows for the visualization of neurons as well as glial cells via established markers in order to determine cell composition and remodeling processes. The methods presented here allow characterizing the SG to gain further information on autonomic dysfunction in mice prone to VA and can be complemented by additional techniques investigating neuronal and glial components of the autonomic nervous system in the heart.

Figure 1&#160;visualizes how to identify and dissect the SG. Figure 1A shows a schematic drawing of the location, while Figure 1B presents the view into&#160;the thorax after removal of the heart-lung-package. The left and right longus colli muscles medial from the SG and the rib cage are important landmarks for orientation. Dissection is performed along the dotted lines between muscles and the first rib. The SG and the sympathetic ...

Watch this Scientific Journal Video about Location, Dissection, and Analysis of the Murine Stellate Ganglion at JoVE.com

Location, Dissection, and Analysis of the Murine Stellate Ganglion

Pathophysiological changes in the cardiac autonomic nervous system, especially in its sympathetic branch, contribute to the onset and maintenance of ventricular arrhythmias. In the present protocol, we show how to characterize murine stellate ganglia to improve the understanding of the underlying molecular and cellular processes.

The autonomic nervous system is a substantial driver of cardiac electrophysiology. Especially&#160;the role of its sympathetic branch is an ongoing matter ...

location-dissection-and-analysis-of-the-murine-stellate-ganglion

Research

JoVE Journal

Medicine

9.9K Views.  EVK Düsseldorf, cNEP, cardiac Neuro- and Electrophysiology Research Consortium. Pathophysiological changes in the cardiac autonomic nervous system, especially in its sympathetic branch, contribute to the onset and maintenance of ventricular arrhythmias. In the present protocol, we show how to characterize murine stellate ganglia to improve the understanding of the underlying molecular and cellular processes.

Video: Location, Dissection, and Analysis of the Murine Stellate Ganglion

Optical Imaging of Neurons in the Crab Stomatogastric Ganglion with Voltage-sensitive Dyes

Voltage-sensitive dye imaging of neurons is a key methodology for the understanding of how neuronal networks are organised and how the simultaneous activity of participating neurons leads to the emergence of the integral functionality of the network. Here we present the methodology of application of this technique to identified pattern generating neurons in the crab stomatogastric ganglion. We demonstrate the loading of these neurons with the fluorescent voltage-sensitive dye Di-8-ANEPPQ and we show how to image the activity of dye loaded neurons using the MiCAM02 high speed and high resolution CCD camera imaging system. We demonstrate the analysis of the recorded imaging data using the BVAna imaging software associated with the MiCAM02 imaging system. The simultaneous voltage-sensitive dye imaging of the detailed activity of multiple neurons in the crab stomatogastric ganglion applied together with traditional electrophysiology techniques (intracellular and extracellular recordings) opens radically new opportunities for the understanding of how central pattern generator neural networks work.

Here we present the methodology for fast and high resolution fluorescent voltage-sensitive dye imaging of detailed activity of neurons in the crab stomatogastric ganglion.

Voltage-sensitive dye imaging of neurons is a key methodology for the understanding of how neuronal networks are organised and how the simultaneous ...

Neuroscience

Homarus Americanus Stomatogastric Nervous System Dissection

With the goal of understanding how nervous systems produce activity and respond to the environment, neuroscientists turn to model systems that exhibit the activity of interest and are accessible and amenable to experimental methods. The stomatogastric nervous system (STNS) of the American lobster (Homarus americanus; also know was the Atlantic or Maine lobster) has been established as a model system for studying rhythm generating networks and neuromodulation of networks. The STNS consists of 3 anterior ganglia (2 commissural ganglia and an oesophageal ganglion), containing modulatory neurons that project centrally to the stomatogastric ganglion (STG). The STG contains approximately 30 neurons that comprise two central pattern generating networks, the pyloric and gastric networks that underlie feeding behaviors in crustaceans1,2. While it is possible to study this system in vivo3, the STNS continues to produce its rhythmic activity when isolated in vitro. Physical isolation of the STNS in a dish allows for easy access to the somata in the ganglia for intracellular electrophysiological recordings and to the nerves of the STNS for extracellular recordings. Isolating the STNS is a two-part process. The first part, dissecting the stomach from the animal, is described in an accompanying video article4. In this video article, fine dissection techniques are used to isolate the STNS from the stomach. This procedure results in a nervous system preparation that is available for electrophysiological recordings.

Homarus Americanus Stomatogastric Nervous System Dissection

We describe the fine dissection of the stomatogastric nervous system from the stomach of the American lobster (Homarus americanus).

With the goal of understanding how nervous systems produce activity and respond to the environment, neuroscientists turn to model systems that exhibit the ...

Biology

Cancer Borealis Stomatogastric Nervous System Dissection

The stomatogastric ganglion (STG) is an excellent model for studying cellular and network interactions because it contains a relatively small number of cells (approximately 25 in C. borealis) which are well characterized. The cells in the STG exhibit a broad range of outputs and are responsible for the motor actions of the stomach. The stomach contains the gastric mill which breaks down food with three internal teeth, and the pylorus which filters the food before it reaches the midgut. The STG produces two rhythmic outputs to control the gastric mill and pylorus known as central pattern generators (CPGs). Each cell in the STG can participate in one or both of these rhythms. These CPGs allow for the study of neuromodulation, homeostasis, cellular and network variability, network development, and network recovery.
The dissection of the stomatogastric nervous system (STNS) from the Jonah crab (Cancer borealis) is done in two parts; the gross and fine dissection. In the gross dissection the entire stomach is dissected from the crab. During the fine dissection the STNS is extracted from the stomach using a dissection microscope and micro-dissection tools (see figure 1). The STNS includes the STG, the oesophageal ganglion (OG), and the commissural ganglia (CoG) as well as the nerves that innervate the stomach muscles. Here, we show how to perform a complete dissection of the STNS in preparation for an electrophysiology experiment where the cells in the STG would be recorded from intracellularly and the peripheral nerves would be used for extracellular recordings. The proper technique for finding the desired nerves is shown as well as our technique of desheathing the ganglion to reveal the somata and neuropil.

Cancer Borealis Stomatogastric Nervous System Dissection

The stomatogastric nervous system (STNS) of the Jonah crab (C. borealis) can be used for electrophysiology, immunohistochemistry, and cell culture studies. The STNS extraction is done in two parts: the gross and fine dissection.

The stomatogastric ganglion (STG) is an excellent model for studying cellular and network interactions because it contains a relatively small number of ...

Analyzing Murine Schwann Cell Development Along Growing Axons

The development of peripheral nerves is an intriguing process. Neurons send out axons to innervate specific targets, which in humans are often more than 100 cm away from the soma of the neuron. Neuronal survival during development depends on target-derived growth factors but also on the support of Schwann cells (SCs). To this end SC ensheath axons from the region of the neuronal soma (or the transition from central to peripheral nervous system) to the synapse or neuromuscular junction. Schwann cells are derivatives of the neural crest and migrate as precursors along emerging axons until the entire axon is covered with SCs. This shows the importance of SC migration for the development of the peripheral nervous system and underlines the necessity to investigate this process. In order to analyze SC development, a setup is needed which next to the SCs also includes their physiological substrate for migration, the axon. Due to intrauterine development in vivo time-lapse imaging, however, is not feasible in placental vertebrates like mouse (mus musculus). To circumvent this, we adapted the superior cervical ganglion (SCG) explant technique. Upon treatment with nerve growth factor (NGF) SCG explants extend axons, followed by SC precursors migrating along the axons from the ganglion to the periphery. The beauty of this system is that the SC are derived from a pool of endogenous SC and that they migrate along their own physiological axons which are growing at the same time. This system is especially intriguing, because the SC development along axons can be analyzed by time-lapse imaging, opening further possibilities to gain insights into SC migration.

Here we describe a Schwann cell (SC) migration assay in which SCs are able to develop along extending axons.

The  development of peripheral nerves is an intriguing process. Neurons send out  axons to innervate specific targets, which in humans are often more than ...

Surgical Technique for Superior Cervical Ganglionectomy in a Murine Model

Growing evidence suggests that the sympathetic nervous system plays an important role in cancer progression. Adrenergic innervation regulates salivary gland secretion, circadian rhythm, macular degeneration, immune function, and cardiac physiology. Murine surgical sympathectomy is a method for studying the effects of adrenergic innervation by allowing for complete, unilateral adrenergic ablation while avoiding the need for repeated pharmacologic intervention and the associated side effects. However, surgical sympathectomy in mice is technically challenging because of the small size of the superior cervical ganglion. This study describes a surgical technique for reliably identifying and resecting the superior cervical ganglion to ablate the sympathetic nervous system. The successful identification and removal of the ganglion are validated by imaging the fluorescent sympathetic ganglia using a transgenic mouse, identifying post-resection Horner's syndrome, staining for adrenergic markers in the resected ganglia, and observing diminished adrenergic immunofluorescence in the target organs following sympathectomy. This model enables future studies of cancer progression as well as other physiological processes regulated by the sympathetic nervous system.

The present protocol describes a mouse model of the ablation of adrenergic innervation by identifying and resecting the superior cervical ganglion.

Growing evidence suggests that the sympathetic nervous system plays an important role in cancer progression. Adrenergic innervation regulates salivary ...

Cancer Research

Optimization of Laser-Capture Microdissection for the Isolation of Enteric Ganglia from Fresh-Frozen Human Tissue

The purpose of this method is to obtain high-integrity RNA samples from enteric ganglia collected from unfixed, freshly-resected human intestinal tissue using laser capture microdissection (LCM). We have identified five steps in the workflow that are crucial for obtaining RNA isolates from enteric ganglia with sufficiently high quality and quantity for RNA-seq. First, when preparing intestinal tissue, each sample must have all excess liquid removed by blotting prior to flattening the serosa as much as possible across the bottom of large base molds. Samples are then quickly frozen atop a slurry of dry ice and 2-methylbutane. Second, when sectioning the tissue, it is important to position cryomolds so that intestinal sections parallel the full plane of the myenteric plexus, thereby yielding the greatest surface area of enteric ganglia per slide. Third, during LCM, polyethylene napthalate (PEN)-membrane slides offer the greatest speed and flexibility in outlining the non-uniform shapes of enteric ganglia when collecting enteric ganglia. Fourth, for distinct visualization of enteric ganglia within sections, ethanol-compatible dyes, like Cresyl Violet, offer excellent preservation of RNA integrity relative to aqueous dyes. Finally, for the extraction of RNA from captured ganglia, we observed differences between commercial RNA extraction kits that yielded superior RNA quantity and quality, while eliminating DNA contamination. Optimization of these factors in the current protocol greatly accelerates the workflow and yields enteric ganglia samples with exceptional RNA quality and quantity.

The goal of this protocol is to obtain high-integrity RNA samples from enteric ganglia isolated from unfixed, freshly-resected human intestinal tissue using laser capture microdissection (LCM). This protocol involves preparing flash-frozen samples of human intestinal tissue, cryosectioning, ethanolic staining and dehydration, LCM, and RNA extraction.

The purpose of this method is to obtain high-integrity RNA samples from enteric ganglia collected from unfixed, freshly-resected human intestinal tissue ...

Dissection of Pelvic Autonomic Ganglia and Associated Nerves in Male and Female Rats

The bilateral major pelvic ganglia (MPG; synonym, pelvic ganglia) are the primary source of postganglionic sympathetic and parasympathetic neurons innervating pelvic organs of rodents; the functionally equivalent structure in humans is the inferior hypogastric plexus. The major pelvic ganglia also provide the route by which lumbar and sacral sensory axons reach the pelvic organs. These complex, mixed ganglia can prove challenging to identify and dissect for further experimental study of normal autonomic mechanisms or to establish preclinical models of disease, injury or visceral pain. Here we describe a protocol to access and visualize these ganglia and their associated nerve tracts. We provide this protocol with schematics for both male and female rats, as the ganglion size and landmarks for identification differ between sexes. The protocol describes removal of the ganglion for in vitro studies, but this method can be integrated into a surgical recovery protocol for experimental interventions (e.g., nerve crush, nerve resection) or for mapping neuronal circuits (e.g., by microinjection of neural tracers). We also demonstrate the primary structures of the ganglion and its associated nerves immediately following dissection and following immunohistochemical staining.

The major pelvic ganglia contain parasympathetic and sympathetic neurons that innervate pelvic organs. Here we describe a dissection method and provide schematics for identification of these ganglia and their associated nerves. These methods can be applied to experimental manipulation of these ganglia in vivo or removal post-mortem for further study.

The bilateral major pelvic ganglia (MPG; synonym, pelvic ganglia) are the primary source of postganglionic sympathetic and parasympathetic neurons ...

Whole Central and Peripheral Nervous System Mice Dissection

Animal models represent the workhorse of the neuroscience field. Despite this, today, there is still no step-by-step protocol to dissect a complete rodent nervous system, nor is there a complete schematic representing it that is freely available. Only methods to harvest the brain, the spinal cord, a specific dorsal root ganglion, and the sciatic nerve (separately) are available. Here, we provide detailed pictures and a schematic of the central and peripheral murine nervous system. More importantly, we outline a robust procedure to perform its dissection. The 30 min pre-dissection step allows isolating the intact nervous system within the vertebra with muscles free of viscera and skin. A 2-4 h dissection follows it under a micro-dissection microscope to expose the spinal cord and the thoracic nerves, and finally peel the whole central and peripheral nervous system off the carcass. This protocol represents a significant step forward in studying the anatomy and pathophysiology of the nervous system globally. For example, the dissected dorsal root ganglions from a neurofibromatosis type I mice model can be further processed for histology to unravel changes in tumor progression.

Here, we present a protocol to complete the dissection of central and peripheral nervous systems of mice. The dissected tissues are further analyzed in downstream applications, such as taking gross pictures or histology.

Animal models represent the workhorse of the neuroscience field. Despite this, today, there is still no step-by-step protocol to dissect a complete rodent ...

Low-input Nucleus Isolation and Multiplexing with Barcoded Antibodies of Mouse Sympathetic Ganglia for Single-nucleus RNA Sequencing

The cardiac autonomic nervous system is crucial in controlling cardiac function, such as heart rate and cardiac contractility, and is divided into sympathetic and parasympathetic branches. Normally, there is a balance between these two branches to maintain homeostasis. However, cardiac disease states such as myocardial infarction, heart failure, and hypertension can induce the remodeling of cells involved in cardiac innervation, which is associated with an adverse clinical outcome.
Although there are vast amounts of data for the histological structure and function of the cardiac autonomic nervous system, its molecular biological architecture in health and disease is still enigmatic in many aspects. Novel technologies such as single-cell RNA sequencing (scRNA-seq) hold promise for the genetic characterization of tissues at single-cell resolution. However, the relatively large size of neurons may impede the standardized use of these techniques. Here, this protocol exploits droplet-based single-nucleus RNA sequencing (snRNA-seq), a method to characterize the biological architecture of cardiac sympathetic neurons in health and disease. A stepwise approach is demonstrated to perform snRNA-seq of the bilateral superior cervical (SCG) and stellate ganglia (StG) dissected from adult mice.
This method enables long-term sample preservation, maintaining an adequate RNA quality when samples from multiple individuals/experiments cannot be collected all at once within a short period of time. Barcoding the nuclei with hashtag oligos (HTOs) enables demultiplexing and the trace-back of distinct ganglionic samples post sequencing. Subsequent analyses revealed successful nuclei capture of neuronal, satellite glial, and endothelial cells of the sympathetic ganglia, as validated by snRNA-seq. In summary, this protocol provides a stepwise approach for snRNA-seq of sympathetic extrinsic cardiac ganglia, a method that has the potential for broader application in studies of the innervation of other organs and tissues.

This protocol describes the detailed, low-input sample preparation for single-nucleus sequencing, including the dissection of mouse superior cervical and stellate ganglia, cell dissociation, cryopreservation, nucleus isolation, and hashtag barcoding.

The cardiac autonomic nervous system is crucial in controlling cardiac function, such as heart rate and cardiac contractility, and is divided into ...

Targeting Mouse Sympathetic Neurons: A Lumbar Sympathectomy Approach

Surgical Lumbar Sympathectomy in Mice

Peripheral nerve injuries are common, and full functional recovery after injury is achieved in only 10% of patients. The sympathetic nervous system plays many critical roles in maintaining bodily homeostasis, but it has rarely been studied in the context of peripheral nerve injury. The extent of postganglionic sympathetic neuronal functions in distal targets in the periphery is currently unclear. To better explore the role of sympathetic innervation of peripheral targets, a surgical &#34;knock-out&#34; model provides an alternative approach. Although this can be achieved chemically, chemical destruction of postganglionic sympathetic neurons can be nonspecific and dose-dependent. The use of a surgical lumbar sympathectomy in mice, once thought to be &#34;virtually not practicable&#34; in small animals, allows for specific targeting of postganglionic sympathetic neurons that innervate the hind limbs. This manuscript describes how to surgically remove the L2-L5 lumbar sympathetic ganglia from a mouse as a survival surgery, which reliably decreases the hind paw sweat response and the number of sympathetic axons in the sciatic nerve.

Author Spotlight: Exploring Plasticity of Sympathetic Neurons

This manuscript presents a protocol for surgically removing the postganglionic lumbar sympathetic neurons from a mouse. This procedure will facilitate a multitude of studies aimed at investigating the role of sympathetic innervation in distal tissue targets.

Peripheral nerve injuries are common, and full functional recovery after injury is achieved in only 10% of patients. The sympathetic nervous system plays ...

Location, Dissection, and Analysis of the Murine Stellate Ganglion

Summary

Explore More Videos

Chapters in this video

Optical Imaging of Neurons in the Crab Stomatogastric Ganglion with Voltage-sensitive Dyes

Homarus Americanus Stomatogastric Nervous System Dissection

Cancer Borealis Stomatogastric Nervous System Dissection

Analyzing Murine Schwann Cell Development Along Growing Axons

Surgical Technique for Superior Cervical Ganglionectomy in a Murine Model

Optimization of Laser-Capture Microdissection for the Isolation of Enteric Ganglia from Fresh-Frozen Human Tissue

Dissection of Pelvic Autonomic Ganglia and Associated Nerves in Male and Female Rats

Whole Central and Peripheral Nervous System Mice Dissection

Low-input Nucleus Isolation and Multiplexing with Barcoded Antibodies of Mouse Sympathetic Ganglia for Single-nucleus RNA Sequencing

Surgical Lumbar Sympathectomy in Mice