Focal Macropatch Recordings of Synaptic Currents from the Drosophila Larval Neuromuscular Junction

Summary

Synaptic currents can be recorded focally from visualized synaptic boutons at the Drosophila third instar larvae neuromuscular junction. This technique enables monitoring the activity of a single synaptic bouton.

Abstract

Drosophila neuromuscular junction (NMJ) is an excellent model system to study glutamatergic synaptic transmission. We describe the technique of focal macropatch recordings of synaptic currents from visualized boutons at the Drosophila larval NMJ. This technique requires customized fabrication of recording micropipettes, as well as a compound microscope equipped with a high magnification, long-distance water immersion objective, differential interference contrast (DIC) optics, and a fluorescent attachment. The recording electrode is positioned on the top of a selected synaptic bouton visualized with DIC optics, epi-fluorescence, or both. The advantage of this technique is that it allows monitoring the synaptic activity of a limited number of sites of release. The recording electrode has a diameter of several microns, and the release sites positioned outside of the electrode rim do not significantly affect the recorded currents. The recorded synaptic currents have fast kinetics and can be readily resolved. These advantages are especially important for the studies of mutant fly lines with enhanced spontaneous or asynchronous synaptic activity.

Introduction

Drosophila is an excellent model system to study the molecular mechanisms controlling synaptic transmission. The neuromuscular system in Drosophila is glutamatergic, and therefore the Drosophila neuromuscular junction (NMJ) can be used to study the conserved features of glutamatergic release. Since Jan and Jan's study¹, the third instar larvae has been broadly used to study evoked and spontaneous synaptic transmission by monitoring excitatory junction potentials (EJPs) or currents (EJCs). EJPs are commonly recorded intracellularly with a sharp glass micro-electrode, and they reflect the activity of the entire NMJ, including all the boutons making synapses at the given muscle fiber.

In contrast, the activity of a limited number of the sites of release can be recorded focally by positioning a micropipette tip near neuronal terminals or synaptic varicosities. This technique was originally employed by Katz and Miledi², and focal extracellular recordings have been successfully employed at several NMJ preparations, including frog^3,4,5, mouse^6,7,8, crustacean^{9,10,11,12,13,14,15,16}, and Drosophila^{17,18,19,20,21,22,23}. This approach was further developed by Dudel, who optimized macropatch recoding electrodes^24,25. In Dudel's implementation, this technique closely matched the loose-patch-clamp method²⁶.

The Drosophila larval NMJ has clearly defined synaptic boutons, and transgenic lines with genetically encoded neuronal fluorescent tags (see Table of Materials) are readily available. These advantages enabled us to record EJCs and mEJCs from a selected synaptic bouton^20,21,22. Here, we describe this technique in detail.

Protocol

1. Fabrication of Recording Electrodes

1. Pulling the glass electrodes
   1. Use the following protocol for the microelectrode puller (see Table of Materials):
      1. Line 1: Heat 510 Pull - Velocity 30 Time 250; Line 2: Heat 490 Pull - Velocity 30 Time 250.
         NOTE: Time units correspond to 0.5 ms per unit; the other units are relative. The value of the heat should be adjusted for every filament after the ramp test is performed.
   2. Use a microscope (35x magnification) to ensure that the inner diameter of the pulled electrode is in the range of 7 - 10 µm (Figure 1A). Store the capillaries in tightly closed containers to prevent dust accumulation.
2. Fire polishing
   1. Fire polish capillaries (80 - 90% of the maximum heat value for 1 - 2 s) using a micro-forge (see Table of Materials). Ensure the final inner diameter of the polished electrode is 5 µm (Figure 1A)²⁷.
3. Bending
   NOTE: Two bends are made in order to position the electrode on the top of the muscle under a high magnification objective.
   1. Use the apparatus shown in Figure 1B. Fix the electrode in the manipulator and position the tip over the filament, not touching it.
   2. Set heat value to 60 - 70% of the maximum and press the pedal of the micro-forge for 1 - 2 s (see Table of Materials) to heat the filament. Use an L-shaped needle to gently pull down the tip of the electrode (Figure 1B enlarged). Make the bend at approximately 90^o (Figure 1C).
   3. Hold the electrode over the flame of the torch by hand using forceps and make the second bend at a distance of 7 - 10 mm from the first bend and at an angle of approximately 120^o (Figure 1C).

Figure 1. Final steps of micropipette fabrication. (A) Electrode tips after pulling and fire polishing. (B.1) The setup for tip bending. (B.2) The boxed area is shown enlarged on the right. The electrode and the filament are fixed so that the electrode tip is positioned slightly above the wire and not touching. (C.1) The recording electrode. (C.2) The boxed area is shown enlarged on the right. The first bend has an angle of approximately 90°, and the distance between the first bend and the tip of the electrode is approximately 1 mm. Scale bar = 3 mm. Please click here to view a larger version of this figure.

2. Additional Preparatory Steps

1. Prepare heamolymph-like (HL3) solution (in mM): 70 NaCl, 5 KCl, 20 MgCl₂, 10 NaHCO₃, 5 trehalose, 115 sucrose, 5 HEPES, and 1 mM CaCl₂; adjust the pH to 7.3 - 7.4. Keep the solution in the refrigerator and make it fresh every week.
2. Make stimulation pipets the same way as recording glass pipets, except there is no need to bend them.
   NOTE: The preparation of stimulation electrodes is described in detail in ²⁸ and ²⁷. The final diameter after fire polishing should be in the range of 5 - 7 µm.
3. Insert a stimulation pipette in a microelectrode holder connected to a syringe.
4. Manufacture dissection plates from small petri dishes (35 x 10 mm) coated with silicone rubber epoxy (see Table of Materials) as described in ²⁸.
   NOTE: Silicone rubber should be completely hardened before use.
5. Pick a wandering third-instar larvae and dissect it as described in^27,28,29,30.
   NOTE: To visualize boutons, use the fly strain CD8-GFP (see Table of Materials)
   1. Using forceps (see Table of Materials), pick the 3^rd instar larvae from a vial.
   2. Pin the larvae, placing the first pin posterior and another pin anterior (close to mouth hooks).
   3. Add HL3 solution.
   4. Make a cut using spring scissors (see Table of Materials) all the way from the top pin to the bottom one on the dorsal side of the larvae.
   5. Pin the larvae fillet, placing 2 additional pins on the left and right sides of the larvae.
   6. Remove the guts and tracheas using forceps.
   7. Cut the nerves just outside the ventral nerve cord using spring scissors.

3. Electrical recordings of EJCs

Figure 2. The recording setup. The sample NMJ pinned to the silicon coated petri dish (arrow) is positioned over the movable stage of the upright compound microscope equipped with epifluorescence capabilities, a high magnification objective, and two micromanipulators. The microscope is stationed on an anti-vibration table. Please click here to view a larger version of this figure.

1. Recording
   1. Place the petri dish with the preparation on the microscope stage (Figure 2). Insert the reference electrode in the bath.
   2. Fill the recording electrode with HL3 solution. Under the 10x objective (see Table of Materials), immerse the electrode into the bath and place it over muscles 6 and 7 of the abdominal segments 2, 3, or 4 using the micromanipulator (see Table of Materials) (Figure 3 A.1 and A.2).
   3. Switch the objective to 60x (see Table of Materials). Focus on the area of interest using either epi-fluorescence or DIC optics. Place the tip of the electrode on top of synaptic bouton (Figure 3 B.1-3).
   4. Press the electrode very gently onto the muscle. Excessive pressure may damage the NMJ or induce an increase in spontaneous synaptic activity. Make sure the tip of the electrode is not clogged- if it is, replace it.
   5. Switch on the amplifier, A/D board, and the computer.
   6. Choose the voltage clamp mode on the amplifier.
   7. Start acquisition software and choose the 'gap-free' mode.
   8. Observe the appearance of mEJCs on the computer screen.
   9. Ensure that the amplitude of the mEJCs is in the range of 0.2 - 0.7 nA.
      NOTE: Smaller EJCs indicate that the recording electrode has defects or that it is not positioned properly.

Figure 3. Visualization of synaptic boutons. (A) A brightfield image of a hemi-segment under 10x magnification (A.1) and the enlarged boxed area showing muscles 6 and 7 (A.2, the arrow marks the recording electrode). Scale bar = 50 µm. (B) Synaptic boutons are visualized in a Drosophila line with a genetically encoded neuronal marker (CD8-GFP) using epi-fluorescence imaging (B.1) or DIC optics (B.2). Images are taken with the 60x objective and the filter cube for GFP imaging (see Table of Materials). Synaptic boutons are marked with arrows, and an overlay of fluorescent and DIC images is shown in B.3. Scale bar = 10 µm. Please click here to view a larger version of this figure.

2. Stimulation
   1. Using a micromanipulator, under a visual control, place the stimulation electrode near the axon innervating abdominal segments 2 - 4.
   2. Apply negative pressure by pulling the piston of the syringe connected to the electrode holder, so that the axon is pulled inside of the electrode (Figure 2).
   3. Turn on the stimulator. Turn the knob on the isolation unit (see Table of Materials) to set a zero current, and then gently increase it, until EJCs appear (or until the threshold is reached).
   4. Perform the stimulation in a suprathreshold regime, with the stimulation current increased approximately twice, compared to the threshold for the observation of EJCs.
      NOTE: In our experience, such stimulation intensity is optimal to avoid action potential failures and action potential firing. For example, if EJCs appear at the stimulation current of 0.2 mA, use a current of 0.4 mA throughout the experiment.
3. Seal resistance
   1. Measure the seal resistance of the recording macropatch electrode by turning the electrode resistance switch of the amplifier to "seal test" position. Observe that the value of seal resistance in GΩ will be displayed in the "current" window.
   2. Make sure the seal resistance is in the range of 0.5 - 2 MΩ. Values out of this range indicate that the electrode is not properly polished or not properly positioned.
   3. Monitor the seal resistance throughout the recording, making sure it remains constant throughout the experiment.

4. Analysis

1. Analyze recordings employing customized software for analysis (see Table of Materials).
   NOTE: Our lab uses in-house software Quantan³¹, which is customized for the detection of EJCs and mEJCs recorded focally (Figure 4). This software includes a Gaussian digital filter and allows the detection of quantal peaks in overlapping multi-quantal events (Figure 4A). Other approaches are described in¹⁷.

Figure 4. Quantal analysis. Detection of mEJCs (A) and EJCs (B) by Quantan software. The event area is marked in green, and peaks are marked by red arrowheads. Please click here to view a larger version of this figure.

Results

Focal macropatch recordings enable monitoring synaptic activity from selected synaptic boutons (Figure 5). When the electrode is positioned on the top of a synaptic bouton (Figure 5A, site 1), the recorded mEJCs (Figure 5C, site 1) have a amplitudes significantly exceeding the noise level and sharp rising phases (at a sub-millisecond range). When the recording electrode is moved away from the synapti...

Discussion

Drosophila represents an advantageous model organism to study synaptic transmission. Several recording configurations have been used at the larval NMJ, including intracellular recordings of synaptic potentials, recordings of synaptic currents with two electrode voltage clamp^33,34, and focal macropatch recordings of synaptic currents described here. The latter technique allows the precise quantification of synaptic transmission at visualized boutons.

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Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Sutter P-97	Sutter instrument	P-97	Microelectrode puller
Narishige MF-830	Narishige	MF-830	Microforge
WPI MF200	WPI	MF200	Microforge
Glass capilaries	WPI	B150-86-10	Glass capilaries
Microtorch 1WG61	Grainer	1WG61	Microtorch
Sylgard 184 Silicone Elastomer Kit	Dow Corning	SYLGARD 184	Silicone for dissection plates preparation
Dissection pins	Amazon	B00J5PMPJA	Pins for larvae positioning
Tweezers	WPIINC	500342	Tweezers for placing pins, removing the guts and tracheas.
Scissors	WPIINC	501778	Scissors for cutting the cuticula of the larvae and nerves.
Olympus BX61WI	Olympus	BX61WI	Upright microscope
Olympus Lumplan FL N 60x	Olympus	UPLFLN 60X	Microscope objective 60X
Olympus UPlan FL N 10x	Olympus	Uplanfl N 10X	Microscope objective 10X
Narishige Micromanipulator	Narishige	MHW-3	Three-axis Water Hydraulic Micromanipulator
npi Electronic GmbH ELC-03XS	npi Electronic GmbH	ELC-03XS	Electrophysiological amplifier
A.M.P.I Master 8	A.M.P.I.	Master 8	Electrical stimulator
A.M.P.I Iso-Flex	A.M.P.I.	Iso-Flex	Stimulus isolator
TMC antivibration table	TMC	63-9090	Antivibration table
TMC Faraday cage	TMC	81-333-90	Faraday cage
Digidata 1322A	Axon Instruments	Digidata 1322A	Digidata
Computer	Dell	Dell Dimension 5150	Computer with Win XP OS
Electrode holder	WPI	MEH3SW	Electrode holder
Optical filter	Omega optical	XF 115-2	Filter cube for Green Fluorescent Protein (GFP) detection
pCLAMP 8	Axon Instruments	8.0.0.81	Software for signal recording
Quantan	In-house software	-	Software for signal processing
Canton-S (Wildtype)	Bloomington Stock Center	64349	Control fly line
cpx SH1	Generous Gift of J.T. Littleton	-	Complexin knock-out fly line with increased spontaneous exocytosis
CD8-GFP	Bloomington Stock Center	5137	Fly line with neuronal fluorescent (GFP) Tag