Method Article

Electrophysiological Investigations of Retinogeniculate and Corticogeniculate Synapse Function

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DOI:

10.3791/59680

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August 7th, 2019

 ,  ,  , 
1Institute of Pathophysiology, University Medical Center of the Johannes Gutenberg University Mainz

In This Article

Summary

Here, we present protocols for the preparation of acute brain slices containing the lateral geniculate nucleus and the electrophysiological investigation of retinogeniculate and corticogeniculate synapses function. This protocol provides an efficient way to study synapses with the high-release and low-release probability in the same acute brain slices.

Abstract

The lateral geniculate nucleus is the first relay station for the visual information. Relay neurons of this thalamic nucleus integrate input from retinal ganglion cells and project it to the visual cortex. In addition, relay neurons receive top-down excitation from the cortex. The two main excitatory inputs to the relay neurons differ in several aspects. Each relay neuron receives input from only a few retinogeniculate synapses, which are large terminals with many release sites. This is reflected by the comparably strong excitation, the relay neurons receive, from retinal ganglion cells. Corticogeniculate synapses, in contrast, are simpler with few release sites and weaker synaptic strength. The two synapses also differ in their synaptic short-term plasticity. Retinogeniculate synapses have a high release probability and consequently display a short-term depression. In contrast, corticogeniculate synapses have a low release probability. Corticogeniculate fibers traverse the reticular thalamic nuclei before entering the lateral geniculate nucleus. The different locations of the reticular thalamic nucleus (rostrally from the lateral geniculate nucleus) and optic tract (ventro-laterally from the lateral geniculate nucleus) allow stimulating corticogeniculate or retinogeniculate synapses separately with extracellular stimulation electrodes. This makes the lateral geniculate nucleus an ideal brain area where two excitatory synapses with very different properties impinging onto the same cell type, can be studied simultaneously. Here, we describe a method to investigate the recording from relay neurons and to perform detailed analysis of the retinogeniculate and corticogeniculate synapse function in acute brain slices. The article contains a step-by-step protocol for the generation of acute brain slices of the lateral geniculate nucleus and steps for recording activity from relay neurons by stimulating the optic tract and corticogeniculate fibers separately.

Introduction

Relay neurons of the lateral geniculate nucleus integrate and relay visual information to the visual cortex. These neurons receive excitatory input from ganglion cells via retinogeniculate synapses, which provide the main excitatory drive for relay neurons. In addition, relay neurons receive excitatory inputs from cortical neurons via corticogeniculate synapses. Moreover, relay neurons receive inhibitory inputs from local interneurons and GABAergic neurons of the nucleus reticularis thalami1. The nucleus reticularis thalami is present like a shield between thalamus and cortex such that fibers projecting from cortex to thalamus and in the opposite direction must go through the nucleus reticularis thalami2.

Retinogeniculate inputs and corticogeniculate inputs display distinct synaptic properties3,4,5,6,7,8. Retinogeniculate inputs form large terminals with multiple release sites9,10. In contrast, corticogeniculate inputs display small terminals with single release sites7. In addition, retinogeniculate synapses efficiently drive action potentials of relay neurons despite constituting only 5−10% of all synapses on relay neurons3,8,11. Corticogeniculate synapses, on the other hand, serve as a modulator of retinogeniculate transmissions by controlling the membrane potential of relay neurons12,13.

These two main excitatory inputs to relay neurons are also functionally different. One prominent difference is the short-term depression of retinogeniculate synapses and the short-term facilitation of corticogeniculate synapses3,5,8. Short-term plasticity refers to a phenomenon in which synaptic strength changes when the synapse is repeatedly active within a time period of few milliseconds to several seconds. Synaptic release probability is an important factor underlying short-term plasticity. Synapses, with a low initial release probability, display short-term facilitation due to the buildup of Ca2+ in the presynapse and consequently an increase in the release probability is observed upon repeated activity. In contrast, synapses with high release probability usually display short-term depression due to the depletion of ready-releasable vesicles14. In addition, desensitization of postsynaptic receptors contributes to the short-term plasticity in some high-release probability synapses8,15. High release probability and desensitization of α-amino-3-hydroxy-5-methyl-4-isoxazolepropionic acid (AMPA) receptors contribute to the prominent short-term depression of retinogeniculate synapses. In contrast, low-release probability underlies the short-term facilitation of corticogeniculate synapses.

In mice, the optic tract enters the dorsal lateral geniculate nucleus (dLGN) from the caudolateral site, whereas corticogeniculate fibers enter the dLGN rostroventrally. The distance between the two inputs allows for the investigation of the individual properties of two very different excitatory inputs impinging onto the same cell. Here, we build on and improve a previously described dissection method in which retinogeniculate and corticogeniculate fibers are preserved in acute brain slices3. We, then, describe the electrophysiological investigation of relay neurons and stimulation of retinogeniculate and corticogeniculate fibers with extracellular stimulation electrodes. Finally, we provide a protocol for the filling of relay neurons with biocytin and subsequent anatomical analysis.

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Protocol

All the experiments were approved by the Governmental Supervisory Panel on Animal Experiments of Rhineland-Palatinate.

1. Solutions

  1. Dissection solution
    1. To reduce excitotoxicity, prepare a choline-based solution to be used during the dissection as presented here (in mM): 87 NaCl, 2.5 KCl, 37.5 choline chloride, 25 NaHCO3, 1.25 NaH2PO4, 0.5 CaCl2, 7 MgCl2, and25 glucose. Prepare the dissection solution less than 1 week before the experiment.
  2. Recording solution
    1. Prepare an artificial cerebral spinal fluid (ACSF) solution containing (in mM): 125 NaCl, 25 NaHCO3, 1.25 NaH2PO4, 2.5 KCl, 2 CaCl2, 1 MgCl2, and 25 glucose. Add 50 µM D-APV and 10 µM SR 95531 hydrobromide to block N-methyl-D-aspartate (NMDA) and GABAA receptors, respectively.
  3. Intracellular solution
    1. Prepare an intracellular solution containing (in mM): 35 Cs-gluconate, 100 CsCl, 10 HEPES, 10 EGTA, and 0.1 D-600 (methoxyverapamil hydrochloride). Adjust the pH to 7.3 with CsOH. Filter, aliquot, and store the stock solution at -20 °C until use.

2. Dissection

  1. Prepare two slice chambers, of which one is filled with 100 mL of the dissection solution and the other with 100 mL of recording solution. Place the two beakers into a water bath (37 °C) and bubble the solutions with carbogen for at least 15 min before the dissection.
  2. Fill a plastic beaker with 250 mL of near ice-cold (but not frozen) dissection solution. Bubble with carbogen at least 15 min before use.
  3. Fill a plastic Petri dish (100 mm x 20 mm), in which the brain dissection will be performed, with the cold dissection solution. Place a piece of filter paper into the lid of the Petri dish.
  4. Cool down the dissection chamber of the vibratome.
  5. Anesthetize a mouse with 2.5% isoflurane, e.g., in the mouse cage. As soon as the mouse does not respond to a tail pinch, decapitate the mouse near the cervical medulla and immerse the head into the ice-cold dissection solution in the base of the Petri dish.
  6. Cut the skin of the head from caudal to nasal and keep it laterally with fingers to expose the skull. To take out the forebrain, first cut the skull along with the posterior-anterior midline, and then cut two more times through the coronal suture and lambdoid suture (Figure 1A).
  7. Remove the skull between the coronal suture and lambdoid suture such that the cerebrum is exposed. Cut the olfactory bulb and separate the forebrain from the midbrain with a fine blade (Figure 1B). Remove the brain from the skull with a thin spatula and place it onto the filter paper in the lid of the Petri dish.
    NOTE: Steps 2.6 and 2.7 should be performed as fast as possible to reduce cell death.
  8. To preserve the integrity of the sensory and cortical inputs to the dLGN in the brain slice, separate the two hemispheres with a parasagittal cut with an angle of 3−5° (Figure 1C,D). Dry the mediolateral planes of the two hemispheres by placing them on the filter paper and then glue them onto the cutting stage with an angle of 10−25° from the horizontal plane (Figure 1E).
  9. Place the stage in the center of the metal buffer tray and gently pour the rest of the ice-cold dissection solution into the buffer tray. Perform this step carefully since a strong pour might remove the pasted brain (Figure 1F).
  10. Place the buffer tray into the ice-filled tray, which helps to maintain the low temperature during dissection. Cut 250 µm slices with a razor blade at a speed of 0.1 mm/s and an amplitude of 1 mm.
  11. Keep slices in the holding chamber filled with oxygenated dissection solution at 34 °C for around 30 min and then allow the slices to recover in the recording solution at 34 °C for another 30 min.
  12. After recovery, remove the slice holding chamber from the water bath and keep slices at room temperature (RT) until used in experiments.

3. Electrophysiology

  1. Pull pipettes using borosilicate glass capillaries and a filament puller. Maintain the resistance of recording pipettes at 3−4 MΩ. Pull stimulating pipettes using the same protocol but break the tip slightly after pulling to increase the diameter. Fill recording pipettes with the intracellular solution and biocytin, while fill stimulating pipettes with the recording solution.
  2. Place the slices into the recording chamber and continuously perfuse the slices with oxygenated recording solution at RT. Check all the slices and select the ones that display an intact optic tract.
  3. Visualize the slice and cells with an upright microscope equipped with infrared differential interference contrast (IR-DIC) video microscopy.
    NOTE: Relay neurons are differentiated from interneurons by their larger soma size and more primary dendrites (branches emerging from the soma). Interneurons display bipolar morphology with a smaller soma.
  4. Place the stimulating pipette onto the slice before patching the cell with the recording pipette. To investigate retinogeniculate synapses, place the stimulating pipette directly onto the optic tract, where the axon fibers from retinal ganglion cells are bundled (Figure 2A). To analyze corticogeniculate synapses, place the stimulating electrode on the nucleus reticularis thalami, which is rostroventrally adjacent to the dLGN (Figure 2B).
  5. Once the recording pipette is immersed into the recording solution, apply a 5 mV voltage step to monitor the pipette resistance. Set the holding potential to 0 mV and cancel the offset potential so that the holding current is 0 pA.
  6. Approach the cell with the recording pipette while applying positive pressure. When the pipette is in direct contact to the cell membrane, release the positive pressure, and set the holding potential to -70 mV. Apply a slight negative pressure to allow the cell membrane to attach to the glass pipette such that a gigaohm seal forms (resistance >1 GΩ). Compensate the pipette capacitance and open the cell by application of negative pressure pulses.
  7. To investigate the synaptic function, apply 0.1 ms current pulses (ca. 30 µA) via the stimulation pipette. If no synaptic responses are observed, the stimulating pipettes may have to be replaced. Be careful during placing the stimulating pipettes to a different position such that the recorded cell is not lost.
    NOTE: In the example recordings shown in Figure 2, synaptic short-term plasticity was investigated by stimulating the optic tract or corticogeniculate fibers twice with 30 ms inter-stimulus intervals. The paired-pulse ratio (PPR) was calculated by dividing the amplitude of the second excitatory postsynaptic current (EPSC) by that of the first EPSC (EPSC2/EPSC1). Each stimulation protocol was repeated 20 times. The EPSC amplitude was measured from average currents of the 20 sweeps. The time interval between each repetition was least 5 s to avoid short-term plasticity induced by the repetitions.
  8. Monitor the series resistance continuously by applying a 5-mV voltage step. Only use the cells with the series resistance smaller than 20 MΩ for analysis.

4. Biocytin labeling

  1. Maintain the whole-cell configuration for at least 5 min to allow the diffusion of biocytin into the distal dendrites.
  2. After recording, gently remove the pipette from the cell so that the soma is not destroyed.
    NOTE: If more than one cell is recorded on one slice, their somas should be sufficiently away from their neighboring cells. Ensure that the dendrites from different cells do not interfere with each other during imaging.
  3. Prepare a 24-well cell culture plate. Fill each well with 300 µL of 4% paraformaldehyde (PFA). Take care to not contaminate anything with PFA that will be in contact with the slices to be recorded.
  4. Transfer the slices from the recording chamber to the PFA-containing plate with a rubber pipette and fix the slices overnight. Ensure that the pipette is always prevented from PFA contamination.
    CAUTION: Always wear gloves and use a chemical hood when manipulating PFA.
  5. After fixing slices overnight in PFA, replace PFA with phosphate-buffered saline (PBS). Store the slices in PBS at 4 °C for future processing (less than 2 weeks).
  6. Wash the slices with fresh PBS 3 times (10 min each wash).
  7. Block nonspecific binding sites by incubating the slices in the blocking solution (0.2% non-ionic surfactant and 5% bovine serum albumin in PBS) for 2 h at RT on an orbital shaker.
  8. Discard the blocking solution. Incubate the slices with streptavidin-Alexa 568 diluted into the blocking solution (1:1,000) at 4 °C overnight on an orbital shaker.
  9. Discard the antibody solution and wash slices 3 times with PBS for 10 min at RT on an orbital shaker. Wash the slices with tap water before mounting.
  10. Put the slices from one mouse on one glass slide. Ensure that the stained cells are present on the top surface of the slices. Absorb the water around the slices with tissues and then leave the slices to dry for approximately 15 min.
  11. Apply two drops of mounting medium on each slice. Mount a coverslip on the slide without producing air bubbles.
  12. Store the labeled slices at 4 °C after visualization with a confocal microscope.

5. Cellular imaging and reconstruction

  1. Scan slices with a confocal microscope and use the associated software for analysis.
  2. Excite the fluorescence at 561 nm.
  3. Image the slices with 0.7 numerical aperture (NA), oil-immersion objective.
  4. Adjust the targeted cell in the middle of the view and apply a 2.5-times magnification.
  5. Render the Z-stack datasets to scan the whole neuron with the following parameters: format = 2,550 x 2,550 pixels, scan frequency = 400 Hz, z number = 40.Voxel size was around 0.1211 x 0.1211 x 1.8463 µm3.
  6. Semi-automatically trace the neurons using a neuronal reconstruction software (e.g., NeuronStudio). An example of a 3D traced relay neuron is shown in Figure 3B.

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Results

The slice preparation of dLGN containing the retinogeniculate and corticogeniculate pathways is shown under a 4x objective (Figure 2). Axons of retinal ganglion cells bundle together in the optic tract (Figure 2). The stimulating pipette was placed on the optic tract to induce retinogeniculate synapse-mediated current (Figure 2A) and on nucleus reticularis thalami to induce corticogeniculate synapses...

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Discussion

We describe an improved protocol based on a previously published method3, which allows for the investigation of the high probability of release retinogeniculate synapses and low probability of release corticogeniculate synapses from the same slice. This is of great importance since these two inputs interact with each other to modulate the visual signal transmission: retinogeniculate inputs are the main excitatory drive of relay neurons, whereas corticothalamic inputs function as a modulator, which...

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Disclosures

The authors have nothing to disclose.

Acknowledgements

This work has been funded by the German Research Foundation (DFG) within the Collaborative Research Center (SFB) 1134 "Functional Ensembles" (J.v.E. and X.C.) and the Research Grant EN948/1-2 (J.v.E.).

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Materials

List of materials used in this article
NameCompanyCatalog NumberComments
Amplifier HEKA ElektronikEPC 10 USB Double patch clamp amplifier
BiocytinSigma-AldrichB4261-250MG
CaCl2EMSURE1.02382.1000
choline chlorideSigma-AldrichC1879-1KG
Confocal Laser Scanning MicroscopeLeica MicrosystemsTCS SP5
CsClEMSURE1.02038.0100
Cs-gluconateSelf-preparedSince there was no commercial Cs-gluconate, we prepared it by ourselves 
D-600 Sigma-AldrichM5644-50MGmethoxyverapamil hydrochloride
D-APV Biotrend BN0085-100NMDA-receptor antagonist
Digital camera for microscopeOlympusXM10
EGTASERVA11290.02
ForeneAbbvie2594.00.00isoflurane
GlucoseSigma-Aldrich49159-1KG
HEPESROTH9105.2
High Current Stimulus IsolatorWorld Precision InstrumentsA385
KClEMSURE1.04936.1000
MgCl2EMSURE1.05833.0250
MicromanipulatorsLuigs & NeumannSM7
MiroscopeOlympusBX51
mounting medium ThermoFisher ScientificP36930Prolong Gold Invitrogen
NaClROTH3957.1
NaH2PO4EMSURE1.06346.1000
NaHCO3EMSURE1.06329.1000
PipetteHilgenberg1807502
PullerSutter P-1000
razor blade Personna 60-0138
Semiautomatic VibratomeLeica  BiosystemsVT1200S
SR 95531 hydrobromide Biotrend AOB5680-10GABAA-receptor antagonist 

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Lateral Geniculate NucleusRetinogeniculate SynapsesCorticogeniculate SynapsesAcute Brain SlicesElectrophysiological RecordingOptic Tract StimulationNucleus Reticularis ThalamiPatch Clamp TechniqueBiocytin LabelingConfocal Microscopy

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