Identification of Specific Sensory Neuron Populations for Study of Expressed Ion Channels

Summary

Afferent sensory neurons signal sensory information from the periphery to the central nervous system. Identifying specific afferent neurons will help in understanding their physiology. We describe a method of retrograde labeling to identify afferent neurons, and study the voltage-gated ion channels in these neurons using patch clamp electrophysiology and immunocytochemistry.

Abstract

Sensory neurons transmit signals from various parts of the body to the central nervous system. The soma for these neurons are located in the dorsal root ganglia that line the spinal column. Understanding the receptors and channels expressed by these sensory afferent neurons could lead to novel therapies for disease. The initial step is to identify the specific subset of sensory neurons of interest. Here we describe a method to identify afferent neurons innervating the muscles by retrograde labeling using a fluorescent dye DiI (1,1'-dioctadecyl-3,3,3',3'-tetramethylindocarbocyanine perchlorate). Understanding the contribution of ion channels to excitation of muscle afferents could help to better control excessive excitability induced by certain disease states such as peripheral vascular disease or heart failure. We used two approaches to identify the voltage dependent ion channels expressed by these neurons, patch clamp electrophysiology and immunocytochemistry. While electrophysiology plus pharmacological blockers can identify functional ion channel types, we used immunocytochemistry to identify channels for which specific blockers were unavailable and to better understand the ion channel distribution pattern in the cell population. These techniques can be applied to other areas of the nervous system to study specific neuronal groups.

Introduction

Dorsal root ganglia (DRG) are comprised of soma from afferent neurons innervating various parts of the body, and important insights can be gained from studying sensory neurons with different innervation targets¹. Various indirect or invasive methods are used to isolate and identify afferent neurons for e.g. injecting the nerve with markers like fluorogold¹, injecting dye into the muscles by surgical method². Of the different dyes that have been successfully used to label neurons and neuronal tracts, fluorescent dyes like DiI are widely used in neuroanatomical tracings owing to their rapid uptake by neuron terminals, long term retention in neurons, and the lack of transfer between neurons³. The afferent neurons labeled with DiI can be easily visualized using a fluorescent microscope for detailed study. However, one limitation is that markers such as DiI can be lost from cells during cell permeabilization needed for immunocytochemistry with intracellular epitopes⁴. Here we describe a method that uses DiI injected into skeletal muscle to identify muscle afferent neurons in the DRG. We also describe a cell permeabilization method that retains DiI in the neuron while permitting antibody access to intracellular epitopes. We demonstrate use of both patch clamp electrophysiology and immunocytochemistry to study these identified neurons, as well as describe the distinct advantages of each technique in studying ion channels that control neuronal excitability. Finally, we describe potential problems that can hinder interpretation of electrophysiological data. We have used these methods to identify muscle and cutaneous afferent neurons and determine the voltage-gated sodium (NaV) channels expressed in these identified neurons⁸. However, these methods can be adapted to a variety of preparations for studying identified subsets of neurons innervating a particular target tissue or brain nucleus.

Protocol

Note: All animal work must be carried out according to institutional and animal care guidelines.

1. Preparation of Animal and Labeling

1. Anesthetize rats: Anesthetize a rat (typically 150-400 g) using an intraperitoneal injection of a mixture of ketamine (50 mg/kg body weight), xylazine (5 mg/kg) and acepromazine (1 mg/kg). Check for reflexes by pinching the foot, wait till there is no response. Since the anesthesia response varies between animals, it is best to determine the effect of the anesthetics by testing pain reflexes.
2. DiI Solution: Weigh DiI powder and dissolve in sterile 100% DMSO to achieve a 1.5% solution (15 mg/ml). Store the solution at room temperature in a dry atmosphere until use.
3. DiI Injections: shave the hair over the calf area on both legs of the anesthetized rat using an electric razor.
   1. Fill a 1 ml sterile syringe (1¼ in 27 G needle) with 200 µl of 1.5% DiI solution. Slowly insert the needle parallel to the long-axis of each gastrocnemius muscle, and inject 100 µl DiI into the muscle while slowly backing the needle out of the muscle (~10 sec) without withdrawing from the muscle.
   2. Prior to withdrawing the needle from the muscle, pull back on the syringe plunger to ensure the dye no longer flows from the tip, wait 10 sec, and then withdraw the needle from the muscle. This step prevents the leakage of DiI from the needle onto the skin, which could label cutaneous afferents.
   3. Repeat for other leg.
   4. Allow 4-5 days for the DiI to be transported from muscle to the DRG.

2. Dissection and Neuronal Isolation

1. Solutions:
   1. Prepare Hank’s Balanced Salt Solution (HBSS) and Earle’s Balanced Salt Solution (EBSS) according to manufacturer’s instructions, filter sterilize and store at 4 °C.
   2. Culture media (MEM Plus): Mix 89 ml minimal essential media (MEM), 10 ml fetal bovine serum (FBS), 1 ml penicillin-streptomycin solution, filter sterilize and store at 4 °C.
   3. Polylysine solution: dissolve poly-L-lysine hydrobromide powder (10 mg/100 ml) in 0.1 M sodium borate solution, pH 8.4, filter sterilize and store aliquots at -20 °C.
2. Coating coverslips
   1. Clean the glass coverslips (12 mm round) in 70% ethanol for 3-4 hr and air dry in sterile culture hood.
   2. Place the dried coverslips in the polylysine solution O/N.
   3. Remove from polylysine solution and wash in sterile distilled water 2x for 5 min each to remove any excess polylysine.
   4. Separate the coverslips, dry in culture hood, and store at 4 ^oC.
3. Setting up for dissection
   1. Place on ice a beaker with 10 ml HBSS, a 35 mm Petri dish and a 100 mm Petri dish.
   2. Weigh out enzymes: 7 mg collagenase, 1 mg of DNAse and 10 mg of trypsin.
   3. Preheat a shaking water bath to 37 ^oC and place into the bath a 15 ml centrifuge tube containing 10 ml of EBSS to warm up.
4. Dissection:
   1. Sacrifice rat according to an IACUC approved protocol. Carbon dioxide was used to euthanize the rat.
   2. Quickly remove the back by cutting open the skin on the back, remove the connective and muscle tissue along the spinal column for better exposure and remove the lumbar section of the vertebral column (end of the thoracic region to the iliac bone; Figure 1).
   3. Place the isolated vertebral column into the 100 mm Petri dish, and using a sterile Pasteur pipette apply chilled HBSS solution to keep the preparation moist and cold.
   4. Cut the muscles from the sides of the vertebral column. Perform a dorsal laminectomy, using rongeurs or scissors, and gently remove the bone enclosing the recesses containing the DRG.
   5. Repeatedly apply ice cold HBSS (~1 ml) during this procedure.
   6. Isolate the DRG by cutting the peripheral and central nerves (leaving 1-2 mm of nerve to facilitate handling of the ganglia)
   7. Place the isolated DRG into the 35 mm Petri dish containing ice-cold HBSS buffer.
   8. Repeat until all L-4 and L-5 DRG have been isolated. Thoracic DRG can be isolated and processed separately as a negative control for DiI labeling.
   9. Place the dish with isolated DRG under a dissection microscope and remove the excess nerves and blood vessels using micro scissors and forceps.
   10. Cut open the DRG for better exposure to the enzymes, but do not desheath the DRG.
5. DRG neuron dissociation:
   1. Add the enzymes into the warm EBSS media (kept in the water bath). Shake briefly to dissolve, and filter sterilize.
   2. Using a sterile Pasteur pipette, place all DRG into the enzyme solution. Minimize the volume of HBSS that is added with DRG since the HBSS will dilute the enzyme mixture.  Gas the flask with 95% O₂ and 5% CO₂ for 60 sec before tightly capping the flask.
   3. Incubate the flask in the shaking water bath set at 37 °C for 60 min at 240 rpm.
   4. At the end of incubation, vigorously shake the flask 50x to dissociate the DRG⁵.
   5. Under sterile conditions, add 5 ml of MEM Plus to the flask to stop the enzymes.
   6. Transfer flask contents to a sterile 15 ml centrifuge tube and centrifuge at 16 x g for 6 min.
   7. Remove and discard the supernatant, add 5 ml of MEM Plus to the sample. Triturate gently with pipette to break up the pellet.
   8. Repeat centrifugation step, remove and discard the supernatant and add 500 µl of MEM Plus. Gently triturate with a 1 ml pipette tip on a pipette to make a cell suspension.
   9. Place one poly-lysine coated glass coverslip into an empty sterile 35 mm dish. Add a drop (~50 µl) of the cell suspension to the center of the coverslip.
   10. Repeat until cell solution is exhausted.
   11. Place the 35 mm dishes into a 37 °C and 5% CO₂ incubator for 1 hr to allow the neurons to adhere to the coverslips.
   12. Add an additional 2 ml of media into each dish and return to the incubator.

3. Patch Clamp Recording

1. Solutions for recording: these solutions are for recording NaV currents. Examples of solutions with differing composition can be found in these references^5-7.
   1. External solution: (in mM) 45 NaCl, 100 N-methyl-d-glucamine (NMG)•Cl, 4 MnCl₂, 10 Na•HEPES and 10 glucose, with pH = 7.4 and osmolarity = 320 mOsm.
   2. Internal solution: (in mM) 104 NMG•Cl, 14 Creatine•PO₄, 6 MgCl₂, 10 NMG•HEPES, 5 Tris•ATP, 10 NMG₂•EGTA, and 0.3 Tris₂•GTP with pH 7.4 and osmolarity = 300 mOsm.
2. Measurement of ionic currents:
   1. Pull recording electrodes from glass capillaries on an electrode puller and heat-polish the tips using a microforge. The resistance of the electrodes is typically 2-3 MΩ
   2. Identify the DiI labeled DRG neurons using a microscope with epifluorescence and a TRITC cube. DiI has an excitation wavelength of 550 nm and emission wavelength of 570 nm.
   3. Fill the glass electrode with internal solution (only filing ~ 1 cm of the electrode tip) and gently tap to remove any trapped bubbles. Place in electrode holder and move to cell using a micromanipulator.
   4. Once the electrode touches the cell, apply gentle suction via the suction tube, until a tight seal is formed ( determined by the increase in electrode resistance).
   5. Clamp the membrane voltage at the desired holding potential (typically -60 to -120 mV).
   6. Obtain the whole-cell patch clamp configuration by applying stronger suction to remove the membrane patch at the tip of the electrode. The transition to whole-cell configuration is observed electrically as an increase in capacitative current^8-10.
   7. Compensate the series resistance using the compensation circuitry of the patch clamp amplifier (use at least 80% compensation)^8,10.

4. Immunocytochemistry

1. Fix the neurons on the coverslips with 4% paraformaldehyde for 1 hr and then permeabilize with 2% Tween 20 in phosphate buffered saline (PBS) for 10 min.
2. Incubate the fixed cells O/N in a blocking solution (normal serum or Bovine Serum Albumin) plus the primary antibody, which is an antibody developed to bind to a specific antigen of interest.
3. Incubate a control set of neurons O/N in blocking solution that lacks the primary antibodies.
4. Wash the coverslips with PBS buffer 3x for 5 min followed by 2 washes of 5 min each with 1% Tween 20 to remove unbound primary antibody.
5. Incubate test and control coverslips with the appropriate fluorescent tagged secondary antibody, which binds to the primary antibody to permit visualization.
6. Wash the coverslips with PBS 3x for 5 min to remove excess secondary antibody.
7. Mount the coverslips on a clean glass slide using mounting media.
8. Apply clear nail polish to edge of the coverslip to fix it place. Once dry, visualize the neurons and capture images using the software accompanying the fluorescence microscope.
   Note: In this work, a Nikon Microscope was used with NIS-elements BR 3.2 software. The exposure time was optimized and kept the same for control and test slides.
9. Measure fluorescence intensity and cell size from individual neurons using imaging software such as ImageJ (rsbweb.nih.gov/ij/index.html).

Results

Using the method described here, we identified muscle afferent neurons in DRG and went on to determine the voltage-gated sodium channels (NaV) expressed by these neurons. DiI labeled muscle afferent neurons (Figure 1C) comprised a small fraction of the total population of neurons in the DRG with an average of 16% of neurons (167/1047) labeled. The quantification was done by first measuring the fluorescence using ImageJ and plotting histograms of the intensity data to determine the threshold for positivel...

Discussion

Muscle afferents originating from triceps surae muscles (e.g. gastrocnemius) have been used in multiple studies to investigate the exercise pressor reflex (EPR)¹³. Given the interest in studying sensory neurons mediating the EPR, the gastrocnemius muscles were selected for dye injection. DiI was chosen due to its lipophilic nature and since it is not lost from the neuron by diffusion through the intact plasma membrane^3,14. Using this method as a guide, one can inject the dye into any target...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
NaV 1.8	Abcam	Ab93616
NaV 1.1 / 1.6/ 1.7 and 1.9	Alamone Labs, Jerusalem, Israel	ASC- 001/ 009 /008 /017
Alexa Fluor secondary antibodies	Invitrogen
Normal goat serum
Fluoro-Gel	Electron Microscopy Sciences	17985