Electrophysiological Investigations of Retinogeniculate and Corticogeniculate Synapse Function

Xufeng Chen; Danni Wang; Marcel Kegel; Jakob von Engelhardt

doi:10.3791/59680

JoVE Journal > Neuroscience

Neuroscience

Electrophysiological Investigations of Retinogeniculate and Corticogeniculate Synapse Function

Published: August 07, 2019

doi:

10.3791/59680

Xufeng Chen¹, Danni Wang¹, Marcel Kegel¹, Jakob von Engelhardt¹

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

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.

Protocol

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

1. Solutions

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 MgCl_2, and₂₅glucose. Prepare the dissection solution less than 1 week before the experiment.
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 GABA_A receptors, respectively.
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

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.
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.
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.
Cool down the dissection chamber of the vibratome.
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.
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).
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.
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).
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).
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.
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.
After recovery, remove the slice holding chamber from the water bath and keep slices at room temperature (RT) until used in experiments.

3. Electrophysiology

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.
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.
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.
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).
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.
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.
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.
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

Maintain the whole-cell configuration for at least 5 min to allow the diffusion of biocytin into the distal dendrites.
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.
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.
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.
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).
Wash the slices with fresh PBS 3 times (10 min each wash).
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.
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.
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.
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.
Apply two drops of mounting medium on each slice. Mount a coverslip on the slide without producing air bubbles.
Store the labeled slices at 4 °C after visualization with a confocal microscope.

5. Cellular imaging and reconstruction

Scan slices with a confocal microscope and use the associated software for analysis.
Excite the fluorescence at 561 nm.
Image the slices with 0.7 numerical aperture (NA), oil-immersion objective.
Adjust the targeted cell in the middle of the view and apply a 2.5-times magnification.
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.
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.

Representative 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-mediated current (Figure 2B), respectively. Of note, axons from cortical neurons to LGN neurons projects from the cortex to thalamus traverse the nucleus reticularis thalami. Corticogenicluate synapses can, therefore, be activated by stimulation in the nucleus reticularis thalami.

The paired-pulse ratio of AMPA receptor-mediated EPSCs is below 1 when stimulating the optic tract with 30 ms inter-stimulus interval, but above 1 when stimulating corticogeniculate fibers with the same inter-stimulus interval (Figure 2C,D). The paired-pulse depression of retinogeniculate synapses is due to a high vesicle release probability and desensitization of postsynaptic AMPA receptors. The paired-pulse facilitation of corticogeniculate synapses is consistent with a low vesicle release probability¹⁶.

Figure 3A shows IR-DIC image showing the soma of a dLGN relay neuron along with the tip of the patch pipette. Biocytin staining enables us to gain a view of the recorded neuron. Different from interneurons, which have bipolar morphology, relay neurons have multipolar dendritic arbors (Figure 3B) containing more than 3 primary dendrites⁸^,¹⁷. Three-dimensional (3D) reconstruction of a biocytin-labeled relay neuron was then generated which shows a radially symmetric dendritic architecture (Figure 3C).

Figure 1: Schemes representing the dissection protocol. (A) Horizontal view of the mouse skull, showing the position of the initial cuts. The first cut was performed along with the sagittal suture, followed by another two cuts along with the coronal suture and lambdoid suture, respectively. Dashed lines represent the incisions. (B) Sagittal view of the whole brain. Dashed lines indicate that the cerebrum is isolated from the olfactory bulb and midbrain. (C-D) These panels show the first cutting angle to separate the two hemispheres from horizontal (C) and coronal (D) view, respectively. (E) Coronal view of one hemisphere on the cutting stage. Dashed lines indicate the slicing direction. l, m, d, and v represent the lateral, medial, dorsal and ventral aspects, respectively, for the hemisphere in panels D and E. (F) Diagram of the dissection chamber with two hemispheres on the cutting stage. The dashed arrow indicates the moving direction of the cutting blade. a, p, and d represent the anterior, posterior, and dorsal aspects of the left hemisphere, respectively. (G) Scheme representing a properly cut slice with a relatively large part of the dLGN and intact preservation of the optic tract. dLGN, dorsal lateral geniculate nucleus; vLGN, ventral lateral nucleus; OT, olfactory bulb; NRT, nucleus reticularis thalami. Panels C, D and G have been modified from Figure 1 of Turner and Salt³. Please click here to view a larger version of this figure.

Figure 2: Slice preparation of dLGN containing the retinogeniculate and corticogeniculate pathways and example recordings. (A-B) These panels show a dLGN slice with preservation of retinogeniculate and corticogeniculate inputs. The stimulation electrode was placed on the optic tract to activate retinogeniculate synapses (A) and on the nucleus reticularis thalami to activate corticogeniculate synapses (B). (C) AMPA receptor-mediated EPSCs in response to stimulation of the optic tract twice with 30 ms inter-stimulus interval. (D) Corticogeniculate synapse-mediated currents with 30 ms inter-stimulus interval. The stimulation artifacts were removed for clarity. Please click here to view a larger version of this figure.

Figure 3: Morphological analysis of a relay neuron. (A) IR-DIC image showing the soma of a dLGN relay neuron with the tip of the patch pipette. (B) Confocal image of a relay neuron labeled with biocytin and visualized with streptavidin-Alexa 568. (C) Three-dimensional (3D) reconstruction of the same neuron, showing a radially symmetric dendritic architecture. Please click here to view a larger version of this figure.

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 influences the gain of retinogeniculate transmission by affecting the state of relay neurons. As expected, we observed that retinogeniculate and corticogeniculate synapses display different short-term plasticity due to the difference in their release probabilities. Additionally, AMPA receptor desensitization also contributes to the strong depression in retinogeniculate synapses⁹^,¹⁵^,¹⁶. We have recently shown that short-term depression is modulated by CKAMP44¹⁶, an AMPA receptor auxiliary protein of the CKAMP family that slows the recovery from desensitization of AMPA receptors¹⁸^,¹⁹^,²⁰. Furthermore, retinogeniculate synapse-mediated current amplitudes are higher than those of corticogeniculate synapse-mediated currents under the same stimulating strength, consistent with the large retinogeniculate synapses with multiple releasing sites, and relatively small corticogeniculate synapses⁷^,²¹.

The slicing protocol is essentially the same as the one developed by Turner and Salt³. Some modifications that were based on our experience improved slice quality. Similar to Hauser et al.²², we used a choline-based instead of a sucrose-based dissection solution. Recovery after dissection was done at 34 °C in the cutting solution for 30 min and then in the recording solution for another 30 min and not at room temperature. Slices were slightly thinner (250 µm instead of 400 µm). We dissected brains using a wedge with an angle of 10−25°, which facilitates and increases the reliability of the slicing procedure.

Recording and stimulation conditions for the investigation of relay neuron synapse function are essentially the same as previously described by Chen and Regehr⁸. Activation of optic tract fibers usually elicits large currents and can be in the range of several nA when all retinogeniculate synapses on one relay neurons are activated²³. To prevent series resistance errors, especially when investigating the maximal current by activating all retinogeniculate synapses on one relay neurons, Chen and Regehr used recording low resistance pipettes (<2 MΩ). However, to investigate synaptic short-term plasticity, it suffices to activate one or few retinal ganglion cell axons, which elicits currents that are in the range of 34−579 pA (unpublished results, Chen et al.). Smaller pipettes with a resistance between 3−4 MΩ can, therefore, be used when investigating retinogeniculate synapse function using weak stimulation of the optic tract. Activation of corticogeniculate synapses elicits relatively small currents¹⁶. Series resistance errors are, therefore, a smaller problem when investigating corticogeniculate synapse function.

We here show that stimulation of retinogeniculate and corticogeniculate synapses can be used to investigate short-term plasticity of AMPA receptor-mediated currents. The same protocol can be applied to record NMDA receptor-mediated current²⁴. In fact, one of the first indications that AMPA receptor desensitization contributes to the short-term plasticity in retinogeniculate synapses came from experiments in which paired-pulse ratios of AMPA receptor-mediated currents were compared with paired-pulse ratios of NMDA receptor-mediated currents. Corticogeniculate synapses were stimulated by positioning the stimulation pipette in the nucleus reticularis thalami because axons of cortical neurons that excite dLGN relay neurons travel across this thalamic nucleus. The same stimulation position can be used to study inhibitory synaptic currents in the dLGN as shown for example by Govindaiah and Cox²⁵.

Relay neurons express GABA_A and GABA_B receptors. The release of GABA activates synaptic GABA_A receptors. GABA_B receptors, which are extrasynaptically localized, are activated when nucleus reticularis thalami are strongly activated for example during burst firing²⁶^,²⁷^,²⁸. Spillover of GABA, which is usually restricted due to GABA uptake by astrocytes, can activate during intense synapse activation the extrasynaptic GABA_B receptors²⁷^,²⁸. We did not block GABA_B receptors because stimulation intensity and frequency were comparably low. However, when investigating corticogeniculate synapse function using intense stimulation protocols it might be preferable to add GABA_B receptors.

Recordings of dLGN relay neurons can readily be performed when using slices that are approximately 2 mm medial from the lateral surface of the brain (start collecting approximately the 8^th of the 250 µm slices during the cutting procedure). In some slices, not both inputs to a given relay neuron can be detected because one of the two pathways are severed close to the relay neuron. In this case, it is usually still possible to investigate retinogeniculate and corticogeniculate synapses in the same slice by selecting different relay neurons for each input. To record retinogeniculate synapse mediated current, ventrally located relay neurons are selected since the optic tract fibers to these cells are more likely preserved than in the dorsally located relay neurons. In contrast, corticogeniculate inputs are more likely preserved onto relay neurons that are located dorsally in the dLGN.

Slice quality determines the reliability of the data. Based on our experience, the following parameters are essential to ensure good slice quality. Cooling and oxygenation are important factors during the dissection procedure. The head of the mouse must be kept in cold solution immediately after the decapitation of the mouse. When taking the brain out of the skull, it should be immersed in ice-cold solution every 3 to 4 s in order to reduce cell death. Similarly, the slicing procedure should be performed at around 4 °C. Moreover, dissection solution and recording solution must be oxygenated at least 15 min before use to maintain sufficient oxygen concentration. In addition, blocking sodium channels can efficiently reduce the neuron activity. Therefore, a dissection solution containing 37.5 mmol choline was used.

Relay neurons display low-threshold spikes, which are generated by the transient Ca²⁺ current²⁹. To block voltage gated Ca²⁺-channels, we added D-600 (methoxyverapamil) to the intracellular solution. D-600 should not be used if the purpose of the study is to investigate low-threshold spikes in relay neurons. The precision of whole-cell voltage clamp recordings is affected by space clamp errors. This technical problem is more relevant for inputs that are far away from the recording electrode (thus for distal synapses)³⁰^,³¹. To minimize the impact of the space clamp error, we used a Cs⁺-based instead of a K⁺-based intracellular solution. Channels that are K⁺permeable (e.g., leak channels) are usually Cs⁺impermeable³². Thus, the use of a Cs⁺-based intracellular solution increases the impedance of the cell.

Stable patch clamp recording depends on the selection of healthy cells. Neurons with round soma shape, dark color or swollen soma should be avoided. Furthermore, relay neurons are distinguished from the local interneurons by their larger soma size and more elaborate primary dendritic arbors. Therefore, we selected cells that have bigger soma size (bigger than 15 µm in diameter) and non-bipolar morphology. The example cell shown in Figure 3B has a symmetrical dendritic architecture and can, therefore, be classified as relay neuron resembling Y-neurons that are for example found in the cat LGN¹⁷.

Series resistance should be as small as possible and maintained constant. Moreover, since the inputs from two directions are preserved in one slice, it is important to get rid of the interference between the two inputs. To avoid activating corticogeniculate fibers when recording retinogeniculate synapse-mediated currents or vice versa, the stimulating pipette should not be placed into the dLGN and the distance between stimulating and recording pipette should be as far as possible. In addition, the long distance between stimulating and recording pipettes requires relatively intact axon preservation. Therefore, a proper cutting angle must be selected for the dissection. In general, only one or two slices with preservation of two inputs can be obtained from each hemisphere.

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.).

Materials

Amplifier	HEKA Elektronik	EPC 10 USB Double patch clamp amplifier
Biocytin	Sigma-Aldrich	B4261-250MG
CaCl₂	EMSURE	1.02382.1000
choline chloride	Sigma-Aldrich	C1879-1KG
Confocal Laser Scanning Microscope	Leica Microsystems	TCS SP5
CsCl	EMSURE	1.02038.0100
Cs-gluconate	Self-prepared		Since there was no commercial Cs-gluconate, we prepared it by ourselves
D-600	Sigma-Aldrich	M5644-50MG	methoxyverapamil hydrochloride
D-APV	Biotrend	BN0085-100	NMDA-receptor antagonist
Digital camera for microscope	Olympus	XM10
EGTA	SERVA	11290.02
Forene	Abbvie	2594.00.00	isoflurane
Glucose	Sigma-Aldrich	49159-1KG
HEPES	ROTH	9105.2
High Current Stimulus Isolator	World Precision Instruments	A385
KCl	EMSURE	1.04936.1000
MgCl₂	EMSURE	1.05833.0250
Micromanipulators	Luigs & Neumann	SM7
Miroscope	Olympus	BX51
mounting medium	ThermoFisher Scientific	P36930	Prolong Gold Invitrogen
NaCl	ROTH	3957.1
NaH₂PO₄	EMSURE	1.06346.1000
NaHCO₃	EMSURE	1.06329.1000
Pipette	Hilgenberg	1807502
Puller	Sutter	P-1000
razor blade	Personna	60-0138
Semiautomatic Vibratome	Leica Biosystems	VT1200S
SR 95531 hydrobromide	Biotrend	AOB5680-10	GABAA-receptor antagonist

References

Guido, W. Development, form, and function of the mouse visual thalamus. Journal of Neurophysiology. 120, 211-225 (2018).
Guillery, R. W., Feig, S. L., Lozsadi, D. A. Paying attention to the thalamic reticular nucleus. Trends in Neurosciences. 21, 28-32 (1998).
Turner, J. P., Salt, T. E. Characterization of sensory and corticothalamic excitatory inputs to rat thalamocortical neurones in vitro. The Journal of Physiology. 510 (3), 829-843 (1998).
Lindstrom, S., Wrobel, A. Frequency dependent corticofugal excitation of principal cells in the cat’s dorsal lateral geniculate nucleus. Experimental Brain Research. 79, 313-318 (1990).
Granseth, B., Ahlstrand, E., Lindstrom, S. Paired pulse facilitation of corticogeniculate EPSCs in the dorsal lateral geniculate nucleus of the rat investigated in vitro. The Journal of Physiology. 544, 477-486 (2002).
Hamos, J. E., Van Horn, S. C., Raczkowski, D., Uhlrich, D. J., Sherman, S. M. Synaptic connectivity of a local circuit neurone in lateral geniculate nucleus of the cat. Nature. 317, 618-621 (1985).
Kielland, A., et al. Activity patterns govern synapse-specific AMPA receptor trafficking between deliverable and synaptic pools. Neuron. 62, 84-101 (2009).
Chen, C., Regehr, W. G. Developmental remodeling of the retinogeniculate synapse. Neuron. 28, 955-966 (2000).
Budisantoso, T., Matsui, K., Kamasawa, N., Fukazawa, Y., Shigemoto, R. Mechanisms underlying signal filtering at a multisynapse contact. The Journal of Neuroscience: The Official Journal of the Society for Neuroscience. 32, 2357-2376 (2012).
Morgan, J. L., Berger, D. R., Wetzel, A. W., Lichtman, J. W. The Fuzzy Logic of Network Connectivity in Mouse Visual Thalamus. Cell. 165, 192-206 (2016).
Usrey, W. M., Reppas, J. B., Reid, R. C. Paired-spike interactions and synaptic efficacy of retinal inputs to the thalamus. Nature. 395, 384-387 (1998).
Steriade, M., Jones, E. G., McCormick, D. A. . Thalamus. , (1997).
Wang, W., Jones, H. E., Andolina, I. M., Salt, T. E., Sillito, A. M. Functional alignment of feedback effects from visual cortex to thalamus. Nature Neuroscience. 9, 1330-1336 (2006).
Zucker, R. S., Regehr, W. G. Short-term synaptic plasticity. Annual Review of Physiology. 64, 355-405 (2002).
Chen, C., Blitz, D. M., Regehr, W. G. Contributions of receptor desensitization and saturation to plasticity at the retinogeniculate synapse. Neuron. 33, 779-788 (2002).
Chen, X., Aslam, M., Gollisch, T., Allen, K., von Engelhardt, J. CKAMP44 modulates integration of visual inputs in the lateral geniculate nucleus. Nature Communications. 9, 261 (2018).
Krahe, T. E., El-Danaf, R. N., Dilger, E. K., Henderson, S. C., Guido, W. Morphologically distinct classes of relay cells exhibit regional preferences in the dorsal lateral geniculate nucleus of the mouse. The Journal of Neuroscience : The Official Journal of the Society for Neuroscience. 31, 17437-17448 (2011).
von Engelhardt, J., et al. CKAMP44: a brain-specific protein attenuating short-term synaptic plasticity in the dentate gyrus. Science. 327, 1518-1522 (2010).
Khodosevich, K., et al. Coexpressed auxiliary subunits exhibit distinct modulatory profiles on AMPA receptor function. Neuron. 83, 601-615 (2014).
Farrow, P., et al. Auxiliary subunits of the CKAMP family differentially modulate AMPA receptor properties. eLife. 4, e09693 (2015).
Rafols, J. A., Valverde, F. The structure of the dorsal lateral geniculate nucleus in the mouse. A Golgi and electron microscopic study. The Journal of Comparative Neurology. 150, 303-332 (1973).
Hauser, J. L., Liu, X., Litvina, E. Y., Chen, C. Prolonged synaptic currents increase relay neuron firing at the developing retinogeniculate synapse. Journal of Neurophysiology. 112, 1714-1728 (2014).
Hooks, B. M., Chen, C. Distinct roles for spontaneous and visual activity in remodeling of the retinogeniculate synapse. Neuron. 52, 281-291 (2006).
Liu, X., Chen, C. Different roles for AMPA and NMDA receptors in transmission at the immature retinogeniculate synapse. Journal of Neurophysiology. 99, 629-643 (2008).
Govindaiah, G., Cox, C. L. Metabotropic glutamate receptors differentially regulate GABAergic inhibition in thalamus. The Journal of Neuroscience: The Official Journal of the Society for Neuroscience. 26, 13443-13453 (2006).
Fogerson, P. M., Huguenard, J. R. Tapping the Brakes: Cellular and Synaptic Mechanisms that Regulate Thalamic Oscillations. Neuron. 92, 687-704 (2016).
Jacobsen, R. B., Ulrich, D., Huguenard, J. R. GABA(B) and NMDA receptors contribute to spindle-like oscillations in rat thalamus in vitro. Journal of Neurophysiology. 86, 1365-1375 (2001).
Kulik, A., et al. Distinct localization of GABA(B) receptors relative to synaptic sites in the rat cerebellum and ventrobasal thalamus. The European Journal of Neuroscience. 15, 291-307 (2002).
Gutierrez, C., Cox, C. L., Rinzel, J., Sherman, S. M. Dynamics of low-threshold spike activation in relay neurons of the cat lateral geniculate nucleus. The Journal of Neuroscience: The Official Journal of the Society for Neuroscience. 21, 1022-1032 (2001).
Armstrong, C. M., Gilly, W. F. Access resistance and space clamp problems associated with whole-cell patch clamping. Methods in Enzymology. 207, 100-122 (1992).
White, J. A., Sekar, N. S., Kay, A. R. Errors in persistent inward currents generated by space-clamp errors: a modeling study. Journal of Neurophysiology. 73, 2369-2377 (1995).
Clay, J. R., Shlesinger, M. F. Analysis of the effects of cesium ions on potassium channel currents in biological membranes. Journal of Theoretical Biology. 107, 189-201 (1984).

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Chen, X., Wang, D., Kegel, M., von Engelhardt, J. Electrophysiological Investigations of Retinogeniculate and Corticogeniculate Synapse Function. J. Vis. Exp. (150), e59680, doi:10.3791/59680 (2019).

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