Optogenetics Identification of a Neuronal Type with a Glass Optrode in Awake Mice

Summary

This work introduces a method to perform an optogenetic single-unit recording reliably from an awake mouse using a custom-made glass optrode.

Abstract

It is a major concern in neuroscience how different types of neurons work in neural circuits. Recent advances in optogenetics have enabled the identification of the neuronal type in in vivo electrophysiological experiments in broad brain regions. In optogenetics experiments, it is critical to deliver the light to the recording site. However, it is often hard to deliver the stimulation light to the deep brain regions from the brain's surface. Especially, it is difficult for the stimulation light to reach the deep brain regions when the optical transparency of the brain surface is low, as is often the case with recordings from awake animals. Here, we describe a method to record spike responses to the light from an awake mouse using a custom-made glass optrode. In this method, the light is delivered through the recording glass electrode so that it is possible to reliably stimulate the recorded neuron with light in the deep brain regions. This custom-made optrode system consists of accessible and inexpensive materials and is easy to assemble.

Introduction

The central nervous system consists of various types of neurons, which have different functions. How these different types of neurons work within the neural circuit is one of the major concerns in neuroscience. However, in many brain regions, it has been impossible to distinguish the neuronal types in in vivo recordings of electrical activities because there is no clear difference in the electrical spike signal itself, with some exceptions. Recent advances in optogenetics have made a breakthrough^1,2. Using transgenic animals in which light-sensitive opsin (e.g., channelrhodopsin-2) is expressed in specific neuronal types, it became possible to distinguish the neuronal types efficiently in in vivo recordings^3,4,5,6. In these animals, the neurons with light-sensitive opsin are excited by giving light stimuli during the electrical recordings, but other neurons are not. The opsin-positive neurons, therefore, are easily distinguished from other neuron types by their responses to light.

In optogenetics experiments, it is critical to deliver the light to the recording site. As a non-invasive method, the light is often directed from the brain's surface. However, because the light's strength reduces as it goes through brain tissue, it is hard to stimulate the deep brain regions from the brain's surface. Especially, it is difficult for the stimulation light to reach the deep brain regions when the optical transparency of the brain surface is low, as is often the case with recordings from awake animals. Electrophysiological experiments have often been performed on anesthetized animals because the body movement causes noise in the recordings. As is well documented, however, anesthesia is known to change the neural responses^7,8,9,10. Thus, it is necessary to use awake animals in order to study neural responses without the artificial effects of anesthesia. Unlike the experiments with anesthetized animals, the electrophysiological recordings are performed after the recovery from surgery in the experiments with awake animals. During the interval between the surgery and the recordings, the tissue exudate often accumulates on the brain surface and makes the optical transparency of the brain surface low.

Here, we describe a method to record single-unit recordings from an awake mouse using a custom-made glass optrode. In this method, the light is delivered through the recording glass electrode so that it is possible to reliably stimulate the recorded neuron with light in deep brain regions. This custom-made optrode system consists of accessible and inexpensive materials and is easy to assemble.

Protocol

All procedures are done in accordance with the guiding principles of the Physiological Society of Japan and with the approval of the Animal Care Committee of Kanazawa Medical University.

1. Construction of the Glass Optrode Holder

NOTE: To build a glass optrode holder, a commercial electrode holder is used (Figure 1A).

1. Gently pull out the steel tube for pressure control from the barrel of the holder.
2. By drilling, broaden the hole of the pin seat side in the barrel of the holder. Make the hole 3 mm in diameter and 12 mm in depth.
3. Put a stainless-steel pipe (3 mm in diameter, 0.5 mm in thickness, and 8 mm in length; Figure 1A2) in the hole.
4. Insert a ceramic split mating sleeve for ⌀2.5 mm ferrules (Figure 1A1) into the hole.
5. Fix the barrel of the electrode holder to an L-shaped rabbet with epoxy adhesive.
6. Make the holes (3 mm in diameter) in the rabbet and attach it to a manipulator with screws.

2. Head Post Installation

1. Prepare a custom-built head post made of a circuit board spacer. Make the columnar circuit board spacer into a cuboidal shape with a milling cutter and cut it into 2 head posts with a saw (Figure 1B). Flatten the bottom of the head post with a milling cutter.
2. Prepare the transgenic animal in which a light-sensitive opsin is expressed in a specific neuron type for the study. In this work, the transgenic mouse (VGAT-ChR2 mice) in which the inhibitory neurons express channelrhodopsin-2 (ChR2)¹¹ is used.
3. Anesthetize the animal with a mixture of 0.3 mg/kg of medetomidine, 4.0 mg/kg of midazolam, and 5.0 mg/kg of butorphanol by intraperitoneal administration. To confirm that the animal is fully anesthetized, test its reactions to tail pinching.
4. Place the mouse in a stereotaxic frame on a heating pad. Clean the stereotaxic frame and the heating pad with 70% alcohol in advance. Place the teeth in the hole of the bite bar, and lightly tighten the nose clamp. Fix both sides of the head using ear bars. When the head is correctly fixed by the ear bars, tighten the nose clamp. Apply an ophthalmic ointment to the eyes.
5. Shave the head skin with small scissors and clean the scalp with a cotton swab of chlorhexidine gluconate. Before the surgery, sterilize all the surgical instruments and a head post with an autoclave (121 °C, 15 min).
6. Cut the scalp along the midline with scissors and push it aside. Make the incision from the back of the head to the eyes (approximately 20 mm). Remove the periosteum with a cotton swab dipped in 70% alcohol and dry the skull.
7. Attach the head post to the manipulator. Position the head post flat on the skull around the bregma using the manipulator.
8. Mix the monomer (4 drops), catalyst (1 drop), and polymer (1 small spoon) of dental cement on a small dish that is chilled in the refrigerator in advance. Put the dental cement (below 1 g) on the frontal and parietal bone of the skull to fix the head post to the skull.
9. After the dental cement becomes hard, remove the mouse from the stereotaxic frame. Put an antibiotic ointment on the exposed skin. Inject the medetomidine antagonist (0.3 mg/kg) and the antibiotics (oxytetracycline; 20 mg/kg). Place and monitor the mouse on the heat pad in a cage until it awakes, and return it to a housing cage.
10. House the animal in an individual housing cage with some enrichment device. Change the animal paper bedding daily to keep the cage clean and prevent infection. Carefully monitor whether the animal shows any sign of discomfort. Apply lidocaine to the wound if any pain is suspected. Administer meloxicam or carprofen once every 24 h for 48 h after both the head post installation and craniotomy surgeries. The local lidocaine can be given in addition if the NSAID is not adequate.

3. Acclimation

1. Two days (minimum) after the recovery from the anesthesia, acclimate the animals to the head-fixed state in the recording chamber. Perform the acclimation sessions for at least 5 days.
2. During the acclimation sessions, place the animal in the recording chamber with the head post fixed to a custom-built clamp. During the session, in order to limit movement, cover the body with a custom-made resin half tube (Figure 1C), made using a 3D printer.
   NOTE: On day 1, the acclimation session should be 5 min long. It is then increased daily to 10, 20, 40, and 60 min for days 2, 3, 4, and 5, respectively.
3. At the end of each session, give the animal a food reward. If the animal struggles continuously during the acclimation, stop the session.

4. Craniotomy

NOTE: After the acclimation, a craniotomy is made over the brain region for recording. The craniotomy is performed in the stereotaxic frame under anesthesia, as with the head post installation. The post-operation procedure is the same as the head post installation. 

1. Before the craniotomy, clean the skull with a cotton swab with chlorhexidine gluconate and 70% alcohol.
2. Carefully scrape the skull over the recording site with a dental drill. When the bone becomes thin enough, cut it with the tip of the scalpel and remove it.
3. Put dental cement around the exposed region in order to strengthen the skull.
4. Cover the exposed brain area with silicone adhesive after the dental cement becomes hard. The post-surgery procedure is as described in step 2.8.

5. Electrophysiological Recording

1. Allow the animal to recover for at least 1 day after the craniotomy before performing the electrophysiological recording. Place the animal in the recording chamber in the same way it was done during the acclimation sessions when the recording starts.
2. Make glass pipettes from borosilicate glass capillaries (OD = 1.5 mm, ID = 0.9 mm, 90.0 mm long) pulled on an electrode puller. Their tip diameter is 2–3 µm, and their resistance is 4–6 MΩ when they are filled with 10 mM PBS. The length of the electrode is 40–50 mm. In some recordings, 2% neurobiotin is added to the 10 mM PBS.
3. Attach the filled glass pipette to the custom-made optrode holder.
4. Put the Ag-Cl coated silver wire (0.2 mm in diameter) into the glass pipette. Connect the silver wire to a pin via a thin coated electric wire. Connect the pin to the headstage of the recording amplifier.
5. Connect the fiber-optic patch cord (core = 960 µm, cladding = 1,000 µm, NA = 0.63) with a zirconia ferrule (OD = 2.5 mm) to the split mating sleeve on the optrode holder. Push the patch cord into the sleeve until the tip of the ferrule contacts the back of the glass pipette. The patch cord delivers the light (wavelength = 465 nm) from LED. The LED light is controlled by a single-channel LED driver.
6. Remove the silicone adhesive over the craniotomy. Put warmed saline (38 °C) on the brain surface periodically to prevent the brain surface from drying during the recording session. If necessary, remove the dura with sharp tweezers.
7. Insert the glass electrode into the brain tissue with a manipulator. Monitor the electrode resistance when it is inserted. Replace the electrode when the resistance is lower than expected because the tip of the electrode may be damaged. At the depth of interest, search and isolate the single unit spikes by adjusting the depth in 2 to 5 µm steps.
8. After the single unit is isolated, deliver the LED light and observe the response to the light stimuli.
9. Record the neural activities after the identification of the cell types. Perform the recordings for 2–3 h. If the recording is made on consecutive days (maximum of 2 days), cover the craniotomy with silicone adhesive. When the recording is finished, and the animal is sacrificed, retrieve the head post and put it in acetone to wash and reuse it.

Results

In Figure 2, we examined the effects of the tip size and the length of the glass pipettes on the light power at the tip of the pipettes (Figure 2A-B). The light power was measured by an optical power meter placed 1 mm away from the tip. The full length was set to 50 ± 2 mm when the tip size varied, while the tip size was set to 2.5 µm when the full length varied. The shank of the glass pipette was set to 8 mm. Th...

Discussion

Optogenetics has become a powerful tool in neuroscience. It has been utilized for identifying specific neuron types in vivo as well as manipulating the activities of specific neuronal pathways. The clarification of the neural activities of different neuronal types promotes the understanding of the mechanism of the neural circuits. Here, we demonstrated a method to deliver the light to the recording site through a glass electrode in the IC of awake VGAT-ChR2 mice.

There are several cri...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Electrode holder	Molecular Device	1-HL-U	pipette holder for microelectrode amplifier
Ceramic split mating sleeve	Thorlabs	ADAF1	f2.5 mm ferrule
Circuit board spacer	Teishin Denki	SPA-320	f8.0 mm, 20.0 mm long
Stereotaxic frame for mice	Narishige	SR-6M-HT	Stereotaxic instruments for mice
Manipulator	Narishige	NA	Manual manipulator
Superbond	Sun Medical	M: 204610557	Dental adhesive resin cement
Form2	Formlabs	NA	3D printer
Kwik-Sil	WPI	KWIK-SIL	Low toxicity silicone adhesive
Borosilicate glass capillaries	Narishige	GD-1.5	OD 1.5 mm, ID 0.9 mm, 90.0 mm long
Fiber-optic patch cord	Doric Lenses	MFP_960/1000/2200-0.63_1m_FCM-ZF2.5	Monofiberoptic patchcord, OD, 2.5 mm, core = 960 mm, cladding = 1000 mm, NA = 0.63
Connectrized LED	Doric Lenses	LEDC-1B_FC	Central wave length = 465 nm, output power = 45 mW (Core 960 mm 0.63 NA )
LED driver	Doric Lenses	LEDRV_1CH_1000	1 ch LED driver, maximum output = 1000 mA
Electrode puller	Narishige	PB-7	Dual-stage glass micropipette puller
Borosilicate glass capillary	Narishige	GD-1.5	Bolosilicate glass capillary, OD, 1.5mm, ID, 0.9 mm, 90.0 mm long
GENTACIN	MSD CO., Ltd	185711173	Antibiotic ointment
Terramycin®-LA	Zoetis	G 333	Oxytetracycline
Tg(Slc32a1- COP4*H134R/EYFP)8Gfng/J	Jackson Labs	#14548	VGAT-ChR2 mice
Multiclamp 700B	Molecular Devices	2500-0157	Microelectrode amplifier