This study was supported by the S&#227;o Paulo Research Foundation [FAPESP grant numbers: 2021/11551-4 (JNS), 2015/20198-5 (TTZ), 2019/21707/1 (RF); and by the Coordena&#231;&#227;o de Aperfei&#231;oamento de Pessoal de N&#237;vel Superior (CAPES) - Finance Code 001&#34; (HRV).

All animal procedures were approved by the Institute of Biomedical Sciences Animals Ethics Committee at the University of S&#227;o Paulo and were performed according to the ethical guidelines adopted by the Brazilian College of Animal Experimentation.
1. Preparation of solutions
<ol>
	<li>Preparation of internal solution 
	NOTE: The internal solution fills the patch-clamp micropipette and will contact the cell&#39;s interior (see an example in Figure 2). Internal solutions may vary depending on the type of activity to be measured33.
	<ol>
		<li>Choose the internal solution considering its experimental purpose and the appropriate record type. To record membrane potential in the current-clamp mode, use the internal solution composed of 120 mM K-gluconate, 1 mM NaCl, 5 mM EGTA, 10 mM HEPES, 1 mM MgCl2, 1 mM CaCl2, 3 mM KOH, 10 mM KCl, and 4 mM (Mg)-ATP. Weigh all the salts according to the desired final volume, as given in Table 1.</li>
		<li>Use enough deionized water to reach 90% of the final volume of the solution. This volume will ensure enough space to adjust the pH and osmolarity.</li>
		<li>After adding and mixing all the ingredients thoroughly, adjust the pH to 7.2-7.3 with 5 M KOH using a pH meter. Use an osmometer to check the osmolarity, which should be around 275-280 mOsm (adjust, if necessary, down only).</li>
		<li>Prepare the internal solution in advance and store at 8 &#176;C. Add the ATP on the day of the experiment. Store the ATP-containing internal solution at -20 &#176;C (1 mL aliquots) for 3-4 months.</li>
	</ol>
	</li>
	<li>Preparation of slicing solution
	<ol>
		<li>Prepare slicing solution containing 238 mM sucrose, 2.5 mM KCl, 26 mM NaHCO3, 1.0 mM NaH2PO4, 10 mM glucose, 1.0 mM CaCl2, and 5.0 mM MgCl2. Weigh all the salts according to the desired final volume, as shown in Table 2. The exact volume of this solution to be prepared will depend on the cutting chamber&#39;s size.</li>
		<li>While mixing all the salts in deionized water, constantly saturate with carbogen (95% O2 and 5% CO2). Attach polyethylene tubing (1.57 mm outer diameter [OD] x 1.14 mm inner diameter [ID]) to a carbogen cylinder to supply carbogen to the slicing solution. Hold the open end of the tube inside the beaker containing the slicing solution.</li>
		<li>After mixing all the ingredients well, adjust the pH to 7.3 with 10% nitric acid using a pH meter. Use an osmometer to check the osmolarity, which should be 290-295 mOsm (adjust, if necessary, down only). Afterward, cool the solution to 0-2 &#176;C.</li>
	</ol>
	</li>
	<li>Prepare aCSF solution for recordings
	<ol>
		<li>Prepare artificial cerebrospinal spinal fluid (aCSF) solution for recordings containing 124 mM NaCl, 2.8 mM KCl, 26 mM NaHCO3, 1.25 mM NaH2PO4, 1.2 mM MgSO4, 5 mM glucose, and 2.5 mM CaCl2. Weigh&#160;all the salts according to the desired final volume, given in Table 3.</li>
		<li>While mixing all the salts in deionized water, constantly saturate with carbogen (95% O2 and 5% CO2), as described in step 1.2.2.</li>
		<li>After adding and mixing all the ingredients, adjust the pH to 7.3 (10% nitric acid can be used) using a pH meter. Use an osmometer to check the osmolarity, which should be 290-300 mOsm. Afterward, pour the aCSF in a beaker and maintain in a water bath at 30 &#176;C.</li>
	</ol>
	</li>
</ol>
2. Brain dissection and slicing
NOTE: Since different brain structures may require cutting in different planes (coronal, sagittal, or horizontal slices), the exact approach for obtaining the slices depends on the brain region of interest. Typically, to study the Kiss1-expressing cells in the AVPV/PeN and ARH (here denominated as AVPV/PeNKisspeptin neurons and ARHkisspeptin neurons; Figure 2A,B), coronal brain slices (200-300 &#181;m) are usually made17,19,20,21,34. The AVPV/PeNKisspeptin neurons are located approximately 0.5 to -0.22 mm from the bregma, whereas ARHkisspeptin neurons are at -1.22 to -2.70 mm. Nuclei location can be determined by using a stereotaxic mouse brain atlas35 or the Allen Mouse Brain Reference Atlas (http://mouse.brain-map.org/). Adult Kiss1-Cre/GFP female (diestrus-stage) and male mice36 were used in this study.
<ol>
	<li>Brain removal
	<ol>
		<li>Prepare the dissection site and the tools needed to extract the brain: decapitation scissors, iris scissors, Castroviejo curved scissors, osteotome, tweezers, spatula, filter paper, Petri dish, razor blade, and cyanoacrylate glue.</li>
		<li>Before making the slices, prepare the bench on which the dissection will be performed, as all subsequent procedures must be performed quickly. Make sure to have access to a slicing device such as a vibratome.</li>
		<li>Prepare a recording chamber to maintain the brain slices before slicing the tissue. Acquire a recording chamber, bath dimensions of 24 mm x 15 mm x 2 mm (L x W x H), from a commercial brand (Table of Materials) or make one in-house. 
		NOTE: An in-house recovery chamber can be fabricated as follows: cut a 24-well plate so that nine wells are available. Glue a nylon screen to the base of the nine wells. With the remainder of the well plate, make a base so that the lower part of the nylon is free. This adapted base can be placed inside a 500 mL beaker containing the aCSF (Supplementary Figure 1).</li>
		<li>After preparing everything, anesthetize the animal with inhaled anesthetic using 4%-5% isoflurane. The anesthesia must be in accordance with a protocol approved by the ethics committee. Shortly after the animal is immobile, perform tail and paw pinch tests to ensure that the animal is deeply anesthetized.</li>
		<li>Quickly decapitate the mice while the heart is still active to augment cell viability. Harvest the brain quickly after decapitation.</li>
		<li>With surgical scissors, make an incision in the skin at the top of the animal&#39;s skull, from caudal to rostral, and remove the scalp from the animal&#39;s head. Next, cut the interparietal plate along the sagittal suture with the iris scissors and remove the occipital bone. Slide the osteotome under the parietal bone and gently pull it out until the brain is exposed.</li>
		<li>After exposing the brain, turn the head upside down, gently lower the brain to visualize the trigeminal nerve on each side, then cut the trigeminal nerve using Castroviejo curved scissors. After visualizing the hypothalamus, identify the optic nerve and cut it gently. 
		NOTE: Be careful when cutting the optic nerve, as pulling it will tear the adjacent hypothalamic area containing the AVPV/PeN nucleus.</li>
		<li>Cut the most anterior portion of the frontal lobe and remove the brain completely. Immediately immerse the brain in the slicing solution until acquiring the slices.</li>
	</ol>
	</li>
	<li>Slicing brain samples
	<ol>
		<li>Place the brain on filter paper (supported on a Petri dish) to dry the excess solution. Then, with a sharp cutting razor blade, perform a coronal cut separating the brainstem with the cerebellum from the rest of the tissue.</li>
		<li>Next, glue the caudal portion of the brain to the base of the vibratome and fill the chamber of the slicing device with the slicing/aCSF solution cooled to 0-2 &#176;C. During the procedure, pack dry ice around the vibratome chamber to keep the slicing solution cold.</li>
		<li>Insert the razor blade into the vibratome and set the device&#39;s appropriate cutting parameters: speed = 3, frequency = 9, and feed = 250 &#956;m. Use an acrylic transfer pipette (inverted Pasteur glass pipette attached to a silicone teat) to transfer the slices to the recovery chamber (described in step 2.1.3) during the tissue-slicing procedure. Wait 60 min for tissue recovery after slice acquisition.</li>
	</ol>
	</li>
</ol>
3. Cell sealing for recording
<ol>
	<li>Ensure that all the pieces of equipment (microscope, amplifier, digitizer, micromanipulator, and others) are turned on before starting the recording.</li>
	<li>Fill the recording chamber, from a commercial brand (Table of Materials), attached to the microscope with the aCSF solution for recordings. Use a perfusion pump to constantly perfuse the aCSF at a rate of 2 mL/min.</li>
	<li>Transfer a brain slice of interest (one at a time) to the recording chamber. Use an acrylic transfer pipette (inverted Pasteur glass pipette attached to a silicone teat) to transfer the hypothalamic slices to the chamber. Use a slice anchor (Table of Materials) to hold the slice so it does not move during the aCSF perfusion.</li>
	<li>Place a slice at the center of the recording chamber attached to the microscope. The slice position is critical to allow a good view of the desired region under the microscope and for a perfect reach of the recording micropipette.</li>
	<li>Use an immersion microscope&#39;s low-power objective lens (10x or 20x) to assist in positioning the slice and locating the region of interest.</li>
	<li>After locating the region of interest, switch the objective lens to the high-power lens (63x) and focus on the tissue level, observing the endogenous fluorescent protein and shapes of the cells in the target region to locate the kisspeptin cells on the surface of the brain slice20.</li>
	<li>When a possible target cell is located, mark it on the computer screen with the mouse cursor or by drawing a format, like a square, over the area of interest. The computer screen mark helps guide the recording micropipette&#39;s position to the cell.</li>
	<li>After determining the exact location of the target cell, lift the objective and introduce the recording micropipette filled with the internal solution. When placing the micropipette in the electrode holder, ensure that the internal solution is in contact with the silver electrode. 
	NOTE: For micropipette preparation, placement, and positioning on the electrode holder, please refer to33.</li>
	<li>Apply positive pressure before submerging the micropipette in the aCSF solution, to prevent debris from entering the micropipette, using a 1-3 mL air-filled syringe connected to the micropipette holder through a polyethylene tubing (&#8776;130 cm longer); apply nearly 100-200 &#956;L of air.</li>
	<li>Using the micromanipulator, guide the micropipette below the center of the objective. Move the buttons on the micromanipulator to guide the micropipette on the X-Y-Z axis toward the cell of interest.</li>
	<li>Adjust the focus to see the tip of the micropipette and bring the focus closer, but not too close, to the slice. Reduce the speed of the micromanipulator and slowly lower the micropipette to the plane of focus. Ensure that the micropipette tip does not abruptly penetrate the slice, but rather slowly descends until it touches the surface of the cell/target region.</li>
	<li>Apply light positive pressure (&#8776;100 &#956;L) with the 1-3 mL air-filled syringe attached to the micropipette holder to clear any debris from the approach path.</li>
	<li>Focus on the target cell and slowly move the micromanipulator on the X-Y-Z axis to bring the micropipette closer to the target cell. When touching the micropipette to the cell, a dimple caused by the pressure applied through the micropipette tip will be observed (Figure 2C).</li>
	<li>After forming the dimple, due to the micropipette&#39;s proximity to the cell, apply weak, brief suction by mouth (1-2 s) through the tube connected to the micropipette holder to generate the seal between the micropipette to the cell (gigaohm seal or gigaseal &#62;1 G&#8486;; Figure 2D). To form the seal, use the voltage-clamp mode on the software. For seal formation details, please refer to33.</li>
	<li>If the seal remains stable (the gigaohm seal should be mechanically stable and without noise interference, determined by observation for about 1 min), set the holding voltage at the closest physiological resting potential of the cell of interest. For kisspeptin hypothalamic neurons, -50 mV is recommended.</li>
	<li>Apply brief suction by mouth (negative pressure) with the micropipette sealed to the cell to break the plasma membrane (Figure 2E). Adequate whole-cell configuration is achieved when suction is performed with sufficient force so that the ruptured membrane does not clog the micropipette and does not attract a sizable portion of the membrane or even the cell.</li>
	<li>Check the system settings manual used. Use the software (see Table of Materials) to digitally check and calculate the series resistance (SR) and the whole-cell capacitance (wcc).</li>
	<li>On voltage-clamp mode, after breaking the cell membrane, enable the whole cell option, and click on the Auto command referring to the whole cell tab. The cell&#39;s SR and wcc will be automatically calculated and instantly displayed by the software. These parameters can also be checked by performing the membrane test with the amplifier mentioned in the Table of Materials33.</li>
	<li>Make sure to check cell viability parameters. For kisspeptin neurons, check that the electrophysiological measurements are: SR &#60; 25 m&#937;, input resistance &#62; 0.3 G&#937;, and holding current absolute value &#60; 30 pA (personal observations and reference21). The mean value of the wcc of AVPV/PeNKisspeptin or ARHkisspeptin neurons is &#8776; 10-12 pF in gonad-intact mice20.</li>
	<li>Monitor the SR and the cell steady-state capacitance during the experiments. Ensure the SR does not change more than 20% during a recording and that the membrane capacitance is stable.</li>
	<li>Check the software settings. Create specific protocols for the recordings according to the type of experiment. To record membrane potential in the current-clamp mode, with equipment mentioned in the Table of Materials, low-pass filter the electrophysiological signals at 2-4 kHz and analyze results offline in a software (see the Table of Materials for software information).</li>
	<li>Once the whole-cell configuration is properly achieved, measure synaptic currents in voltage-clamp mode (Figure 2G). Record changes in resting membrane potential (RMP) and induced RMP variations in the current-clamp mode (Figure 2H). Changes in RMP, such as depolarization of the cell membrane, can be induced by administering a known drug/neurotransmitter to the bath (described in step 3.2), as illustrated in Figure 1. 
	NOTE: In current-clamp mode, positive or negative current can be injected to hold the membrane voltage at a desired voltage. For kisspeptin neurons, we usually set zero current injection (I = 0) to record the spontaneous variation of the membrane potential.</li>
</ol>

No conflicts of interest to be declared.

The development of the whole-cell patch-clamp technique had a significant impact on the scientific community, being considered of paramount importance for developing scientific research and enabling several discoveries. Its impact on science was enough to culminate in the Nobel Prize in Medicine in 1991, as this discovery opened the door to a better understanding of how ion channels function under physiological and pathological conditions, as well as the identification of potential targets for therapeutic agents<sup clas...

Hodgkin and Huxley made the first intracellular record of an action potential described in several scientific studies. This recording was performed on the squid axon, which has a large diameter (~500 &#181;m), allowing a microelectrode to be placed inside the axon. This work provided great possibilities for scientific research, later culminating in the creation of the voltage-clamp mode, which was used to study the ionic basis of action potential generation1,2,3,4,5,6,7,8. Over the years, the technique has been improved, and it has become widely applied in scientific research6,9. The invention of the patch-clamp technique, which took place in the late 1970s through studies initiated by Erwin Neher and Bert Sakmann, allowed researchers to record single ion channels and intracellular membrane potentials or currents in virtually every type of cell using only a single electrode9,10,11,12. Patch-clamp recordings can be made on a variety of tissue preparations, such as cultured cells or tissue slices, in either voltage-clamp mode (holding the cell membrane at a set voltage allowing the recording of, for example, voltage-dependent currents and synaptic currents) or current-clamp mode (allowing the recording of, for example, changes in resting membrane potential induced by ion currents, action potentials, and postsynaptic potential frequency).
The use of the patch-clamp technique made several notable discoveries possible. Indeed, the seminal findings on the electrophysiological properties of hypothalamic kisspeptin neurons located at the anteroventral periventricular and rostral periventricular nuclei (AVPV/PeNKisspeptin), also known as the rostral periventricular area of the third ventricle (RP3V), and the arcuate nucleus of the hypothalamus (ARHkisspeptin)13,14,15 are of particular interest. In 2010, Ducret et al. performed the first recordings of AVPV/PeNKisspeptinneurons in mice using another electrophysiological tool, the loose-cell patch-clamp technique. These studies provided an electrical description of AVPV/PeNKisspeptin neurons and demonstrated that their firing patterns are estrous cycle-dependent16. In 2011, Qiu et al. used the whole cell patch-clamp technique to demonstrate that ARHkisspeptin neurons express endogenous pacemaker currents17. Subsequently, Gottsch et al. showed that kisspeptin neurons exhibit spontaneous activity and express both h-type (pacemaker) and T-type calcium currents, suggesting that ARHkisspeptin neurons share electrophysiological properties with other central nervous system pacemaker neurons18. Additionally, it has been demonstrated that ARHkisspeptin neurons exhibit sexually dimorphic firing rates and that AVPV/PeNKisspeptin neurons exhibit a bimodal resting membrane potential (RMP) influenced by ATP-sensitive potassium channels (KATP)19,20. Furthermore, it was established that gonadal steroids positively affect the spontaneous electrical activity of the kisspeptin neurons in mice19,20,21. The first works that study kisspeptin neurons&#39; electrophysiological properties are mentioned16,17,18,19,20. Since then, many studies have used the whole-cell patch-clamp technique to demonstrate which factors/neuromodulators are sufficient to modulate the electrical activity of kisspeptin neurons (Figure 1)17,21,22,23,24,25,26,27,28,29,30,31,32.
Given the importance of this technique for the study of neurons that are required for reproduction, among other cell types not covered here, this article describes the basic steps for the development of the whole-cell patch-clamp technique, such as preparing the solutions, dissecting and slicing the brain, and performing the seal of the cell membrane for recordings. Moreover, relevant issues about the technique are discussed, such as its advantages, technical limitations, and important variables that must be controlled for optimal experimental performance.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Compounds for aCSF, internal and slicing solutions</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>ATP</td>
			<td>Sigma Aldrich/various</td>
			<td>A9187</td>
			<td></td>
		</tr>
		<tr>
			<td>CaCl2</td>
			<td>Sigma Aldrich/various</td>
			<td>C7902</td>
			<td></td>
		</tr>
		<tr>
			<td>D-(+)-Glucose</td>
			<td>Sigma Aldrich/various</td>
			<td>G7021</td>
			<td></td>
		</tr>
		<tr>
			<td>EGTA</td>
			<td>Sigma Aldrich/various</td>
			<td>O3777</td>
			<td></td>
		</tr>
		<tr>
			<td>HEPES</td>
			<td>Sigma Aldrich/various</td>
			<td>H3375</td>
			<td></td>
		</tr>
		<tr>
			<td>KCL</td>
			<td>Sigma Aldrich/various</td>
			<td>P5405</td>
			<td></td>
		</tr>
		<tr>
			<td>K-gluconate</td>
			<td>Sigma Aldrich/various</td>
			<td>G4500</td>
			<td></td>
		</tr>
		<tr>
			<td>KOH</td>
			<td>Sigma Aldrich/various</td>
			<td>P5958</td>
			<td></td>
		</tr>
		<tr>
			<td>MgCl2</td>
			<td>Sigma Aldrich/various</td>
			<td>M9272</td>
			<td></td>
		</tr>
		<tr>
			<td>MgSO4</td>
			<td>Sigma Aldrich/various</td>
			<td>230391</td>
			<td></td>
		</tr>
		<tr>
			<td>NaCl</td>
			<td>Sigma Aldrich/various</td>
			<td>S5886</td>
			<td></td>
		</tr>
		<tr>
			<td>NaH2PO4&#160;</td>
			<td>Sigma Aldrich/various</td>
			<td>S5011</td>
			<td></td>
		</tr>
		<tr>
			<td>NaHCO3</td>
			<td>Sigma Aldrich/various</td>
			<td>S5761</td>
			<td></td>
		</tr>
		<tr>
			<td>nitric acid</td>
			<td>Sigma Aldrich/various</td>
			<td>225711</td>
			<td>CAUTION</td>
		</tr>
		<tr>
			<td>Sucrose</td>
			<td>Sigma Aldrich/various</td>
			<td>S1888</td>
			<td></td>
		</tr>
		<tr>
			<td>Equipments</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Air table</td>
			<td>TMC</td>
			<td>63-534</td>
			<td></td>
		</tr>
		<tr>
			<td>Amplifier</td>
			<td>Molecular Devices</td>
			<td>Multiclamp 700B</td>
			<td></td>
		</tr>
		<tr>
			<td>Computer</td>
			<td>various</td>
			<td>-</td>
			<td></td>
		</tr>
		<tr>
			<td>DIGIDATA 1440 LOW-NOISE DATA ACQUISITION SYSTEM</td>
			<td>Molecular Devices</td>
			<td>DD1440</td>
			<td></td>
		</tr>
		<tr>
			<td>Digital peristaltic pump</td>
			<td>Ismatec</td>
			<td>ISM833C&#160;</td>
			<td></td>
		</tr>
		<tr>
			<td>Faraday cage</td>
			<td>TMC</td>
			<td>81-333-03</td>
			<td></td>
		</tr>
		<tr>
			<td>Imaging Camera</td>
			<td>Leica</td>
			<td>DFC 365 FX</td>
			<td></td>
		</tr>
		<tr>
			<td>Micromanipulator</td>
			<td>Sutter Instruments</td>
			<td>Roe-200</td>
			<td></td>
		</tr>
		<tr>
			<td>Micropipette Puller</td>
			<td>Narishige</td>
			<td>PC-10</td>
			<td></td>
		</tr>
		<tr>
			<td>Microscope</td>
			<td>Leica</td>
			<td>DM6000 FS</td>
			<td></td>
		</tr>
		<tr>
			<td>Osteotome</td>
			<td>Bonther equipamentos &#38; Tecnologia/various</td>
			<td>128</td>
			<td></td>
		</tr>
		<tr>
			<td>Recovery chamber</td>
			<td>Warner Instruments/Harvard apparatus</td>
			<td>-</td>
			<td>can be made in-house</td>
		</tr>
		<tr>
			<td>Recording chamber</td>
			<td>Warner Instruments</td>
			<td>640277</td>
			<td></td>
		</tr>
		<tr>
			<td>Spatula</td>
			<td>Fisher Scientific /various</td>
			<td>FISH-14-375-10; FISH-21-401-20</td>
			<td></td>
		</tr>
		<tr>
			<td>Vibratome&#160;</td>
			<td>Leica</td>
			<td>VT1000 S</td>
			<td></td>
		</tr>
		<tr>
			<td>Water Bath&#160;</td>
			<td>Fisher Scientific /various</td>
			<td>Isotemp</td>
			<td></td>
		</tr>
		<tr>
			<td>Software and systems</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>AxoScope 10 software</td>
			<td>Molecular Devices</td>
			<td>-</td>
			<td>Commander Software</td>
		</tr>
		<tr>
			<td>LAS X wide field system</td>
			<td>Leica</td>
			<td>-</td>
			<td>Image acquisition and analysis</td>
		</tr>
		<tr>
			<td>MultiClamp 700B</td>
			<td>Molecular Devices</td>
			<td>MULTICLAMP 700B</td>
			<td>Commander Software</td>
		</tr>
		<tr>
			<td>PCLAMP 10 SOFTWARE FOR WINDOWS</td>
			<td>Molecular Devices</td>
			<td>Pclamp 10 Standard</td>
			<td></td>
		</tr>
		<tr>
			<td>Tools</td>
			<td></td>
			<td></td>
			<td></td>
		</tr>
		<tr>
			<td>Ag/AgCl electrode, pellet, 1.0 mm</td>
			<td>Warner Instruments</td>
			<td>64-1309</td>
			<td></td>
		</tr>
		<tr>
			<td>Curved hemostatic forcep</td>
			<td>various</td>
			<td>-</td>
			<td></td>
		</tr>
		<tr>
			<td>cyanoacrylate glue</td>
			<td>LOCTITE/various</td>
			<td>-</td>
			<td></td>
		</tr>
		<tr>
			<td>Decapitation scissors</td>
			<td>various</td>
			<td>-</td>
			<td></td>
		</tr>
		<tr>
			<td>Filter paper</td>
			<td>various</td>
			<td>-</td>
			<td></td>
		</tr>
		<tr>
			<td>Glass capillaries (micropipette)</td>
			<td>World Precision Instruments, Inc</td>
			<td>TW150F-4</td>
			<td></td>
		</tr>
		<tr>
			<td>Iris scissors</td>
			<td>Bonther equipamentos &#38; Tecnologia/various</td>
			<td>65-66</td>
			<td></td>
		</tr>
		<tr>
			<td>Pasteur glass pipette&#160;</td>
			<td>Sigma Aldrich/various</td>
			<td>CLS7095B9-1000EA</td>
			<td></td>
		</tr>
		<tr>
			<td>Petri dish</td>
			<td>various</td>
			<td>-</td>
			<td></td>
		</tr>
		<tr>
			<td>Polyethylene tubing&#160;</td>
			<td>Warner Instruments</td>
			<td>64-0756</td>
			<td></td>
		</tr>
		<tr>
			<td>Razor blade for brain dissection</td>
			<td>TED PELLA</td>
			<td>TEDP-121-1</td>
			<td></td>
		</tr>
		<tr>
			<td>Razor blade for the vibratome</td>
			<td>TED PELLA</td>
			<td>TEDP-121-9</td>
			<td></td>
		</tr>
		<tr>
			<td>Scissors</td>
			<td>Bonther equipamentos &#38; Tecnologia/various</td>
			<td>71-72, 48,49;&#160;</td>
			<td></td>
		</tr>
		<tr>
			<td>silicone teat</td>
			<td>various</td>
			<td>-</td>
			<td></td>
		</tr>
		<tr>
			<td>Slice Anchor&#160;</td>
			<td>Warner Instruments</td>
			<td>64-0246</td>
			<td></td>
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		<tr>
			<td>Syringe filters</td>
			<td>Merck Millipore Ltda</td>
			<td>SLGVR13SL</td>
			<td>Millex-GV 0.22 &#956;m</td>
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		<tr>
			<td>Tweezers</td>
			<td>Bonther equipamentos &#38; Tecnologia/various</td>
			<td>131, 1518</td>
			<td></td>
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hypothalamic kisspeptin neurons as a target for whole-cell patch-clamp recordings

Kisspeptins are essential for the maturation of the hypothalamic-pituitary-gonadal (HPG) axis and fertility. Hypothalamic kisspeptin neurons located in the anteroventral periventricular nucleus and rostral periventricular nucleus, as well as the arcuate nucleus of the hypothalamus, project to gonadotrophin-releasing hormone (GnRH) neurons, among other cells. Previous studies have demonstrated that kisspeptin signaling occurs through the Kiss1 receptor (Kiss1r), ultimately exciting GnRH neuron activity. In humans and experimental animal models, kisspeptins are sufficient for inducing GnRH secretion and, consequently, luteinizing hormone (LH) and follicle stimulant hormone (FSH) release. Since kisspeptins play an essential role in reproductive functions, researchers are working to assess how the intrinsic activity of hypothalamic kisspeptin neurons contributes to reproduction-related actions and identify the primary neurotransmitters/neuromodulators capable of changing these properties. The whole-cell patch-clamp technique has become a valuable tool for investigating kisspeptin neuron activity in rodent cells. This experimental technique allows researchers to record and measure spontaneous excitatory and inhibitory ionic currents, resting membrane potential, action potential firing, and other electrophysiological properties of cell membranes. In the present study, crucial aspects of the whole-cell patch-clamp technique, known as electrophysiological measurements that define hypothalamic kisspeptin neurons, and a discussion of relevant issues about the technique, are reviewed.

To study the possible effects of human recombinant growth hormone (hGH) on the activity of hypothalamic kisspeptin neurons, we performed whole-cell patch-clamp recordings in brain slices and assessed whether this hormone causes acute changes in the activity of AVPV/PeNKisspeptin and ARHkisspeptin neurons. Adult Kiss1-Cre/GFP female (diestrus-stage) and male mice36 were used in this study.&#160;Gonad-intact animals were selected for the experiments, since the properties of the...

Watch this Scientific Journal Video about Hypothalamic Kisspeptin Neurons as a Target for Whole-Cell Patch-Clamp Recordings at JoVE.com

Hypothalamic Kisspeptin Neurons as a Target for Whole-Cell Patch-Clamp Recordings

Here, we present a protocol to perform a whole-cell patch-clamp on brain slices containing kisspeptin neurons, the primary modulator of gonadotrophin-releasing hormone (GnRH) cells. By adding knowledge about kisspeptin neuron activity, this electrophysiological tool has served as the basis for significant advancements in the neuroendocrinology field over the last 20 years.

Kisspeptins are essential for the maturation of the hypothalamic-pituitary-gonadal (HPG) axis and fertility. Hypothalamic kisspeptin neurons located in ...

hypothalamic-kisspeptin-neurons-as-target-for-whole-cell-patch-clamp

Research

JoVE Journal

Neuroscience

1.8K Views.  Universidade de Sao Paulo. Here, we present a protocol to perform a whole-cell patch-clamp on brain slices containing kisspeptin neurons, the primary modulator of gonadotrophin-releasing hormone (GnRH) cells. By adding knowledge about kisspeptin neuron activity, this electrophysiological tool has served as the basis for significant advancements in the neuroendocrinology field over the last 20 years.

Video: Hypothalamic Kisspeptin Neurons as a Target for Whole-Cell Patch-Clamp Recordings

Patch Clamp Recordings from Mouse Retinal Neurons in a Dark-adapted Slice Preparation

Our visual experience is initiated when the visual pigment in our retinal photoreceptors absorbs photons of light energy and initiates a cascade of intracellular events that lead to closure of cyclic-nucleotide-gated channels in the cell membrane. The resulting change in membrane potential leads in turn to reductions in the amount of neurotransmitter release from both rod and cone synaptic terminals. To measure how the light-evoked change in photoreceptor membrane potential leads to downstream activity in the retina, scientists have made electrophysiological recordings from retinal slice preparations for decades1,2. In the past these slices have been cut manually with a razor blade on retinal tissue that is attached to filter paper; in recent years another method of slicing has been developed whereby retinal tissue is embedded in low gelling temperature agar and sliced in cool solution with a vibrating microtome3,4. This preparation produces retinal slices with less surface damage and very robust light-evoked responses. Here we document how this procedure can be done under infrared light to avoid bleaching the visual pigment.

Here we describe a procedure for generating dark-adapted slices of the mouse retina for electrophysiological recordings.

Our visual experience is initiated when the visual pigment in our retinal photoreceptors absorbs photons of light energy and initiates a cascade of ...

Paired Patch Clamp Recordings from Motor-neuron and Target Skeletal Muscle in Zebrafish

Larval zebrafish represent the first vertebrate model system to allow simultaneous patch clamp recording from a spinal motor-neuron and target muscle. This is a direct consequence of the accessibility to both cell types and ability to visually distinguish the single segmental CaP motor-neuron on the basis of morphology and location. This video demonstrates the microscopic methods used to identify a CaP motor-neuron and target muscle cells as well as the methodologies for recording from each cell type. Identification of the CaP motor-neuron type is confirmed by either dye filling or by the biophysical features such as action potential waveform and cell input resistance. Motor-neuron recordings routinely last for one hour permitting long-term recordings from multiple different target muscle cells. Control over the motor-neuron firing pattern enables measurements of the frequency-dependence of synaptic transmission at the neuromuscular junction. Owing to a large quantal size and the low noise provided by whole cell voltage clamp, all of the unitary events can be resolved in muscle. This feature permits study of basic synaptic properties such as release properties, vesicle recycling, as well as synaptic depression and facilitation. The advantages offered by this in vivo preparation eclipse previous neuromuscular model systems studied wherein the motor-neurons are usually stimulated by extracellular electrodes and the muscles are too large for whole cell patch clamp. The zebrafish preparation is amenable to combining electrophysiological analysis with a wide range of approaches including transgenic lines, morpholino knockdown, pharmacological intervention and in vivo imaging. These approaches, coupled with the growing number of neuromuscular disease models provided by mutant lines of zebrafish, open the door for new understanding of human neuromuscular disorders.

Larval zebrafish represent the first vertebrate model system to allow simultaneous patch clamp recording from a spinal motor-neuron and target skeletal muscle. This video demonstrates the microscopic methods used to identify a segmental CaP motor-neuron and target muscle cells as well as the methodologies for recording from each cell type.

Larval zebrafish represent the first vertebrate model system to allow simultaneous patch clamp recording from a spinal motor-neuron and target muscle.  ...

Whole Cell Patch Clamp for Investigating the Mechanisms of Infrared Neural Stimulation

It has been demonstrated in recent years that pulsed, infrared laser light can be used to elicit electrical responses in neural tissue, independent of any further modification of the target tissue. Infrared neural stimulation has been reported in a variety of peripheral and sensory neural tissue in vivo, with particular interest shown in stimulation of neurons in the auditory nerve. However, while INS has been shown to work in these settings, the mechanism (or mechanisms) by which infrared light causes neural excitation is currently not well understood. The protocol presented here describes a whole cell patch clamp method designed to facilitate the investigation of infrared neural stimulation in cultured primary auditory neurons. By thoroughly characterizing the response of these cells to infrared laser illumination in vitro under controlled conditions, it may be possible to gain an improved understanding of the fundamental physical and biochemical processes underlying infrared neural stimulation.

Infrared nerve stimulation has been proposed as an alternative to electrical stimulation in a range of nerve types, including those associated with the auditory system. This protocol describes a patch clamp method for studying the mechanism of infrared nerve stimulation in a culture of primary auditory neurons.

It has been  demonstrated in recent years that pulsed, infrared laser light can be used to  elicit electrical responses in neural tissue, independent of ...

Isolation of Sensory Neurons of Aplysia californica for Patch Clamp Recordings of Glutamatergic Currents

The marine gastropod mollusk Aplysia californica has a venerable history as a model of nervous system function, with particular significance in studies of learning and memory. The typical preparations for such studies are ones in which the sensory and motoneurons are left intact in a minimally dissected animal, or a technically elaborate neuronal co-culture of individual sensory and motoneurons. Less common is the isolated neuronal preparation in which small clusters of nominally homogeneous neurons are dissociated into single cells in short term culture. Such isolated cells are useful for the biophysical characterization of ion currents using patch clamp techniques, and targeted modulation of these conductances. A protocol for preparing such cultures is described. The protocol takes advantage of the easily identifiable glutamatergic sensory neurons of the pleural and buccal ganglia, and describes their dissociation and minimal maintenance in culture for several days without serum.

Isolation of Sensory Neurons of Aplysia californica for Patch Clamp Recordings of Glutamatergic Currents

We describe the dissection of the nervous system of the marine sea hare Aplysia after anesthesia, the isolation of neurons for short term-tissue culture, and recordings of single cell ion currents via the patch clamp technique.

The marine gastropod mollusk Aplysia californica has a venerable  history as a model of nervous system function, with particular significance in  studies ...

Whole-cell Patch-clamp Recordings from Morphologically- and Neurochemically-identified Hippocampal Interneurons

GABAergic inhibitory interneurons play a central role within neuronal circuits of the brain. Interneurons comprise a small subset of the neuronal population (10-20%), but show a high level of physiological, morphological, and neurochemical heterogeneity, reflecting their diverse functions. Therefore, investigation of interneurons provides important insights into the organization principles and function of neuronal circuits. This, however, requires an integrated physiological and neuroanatomical approach for the selection and identification of individual interneuron types. Whole-cell patch-clamp recording from acute brain slices of transgenic animals, expressing fluorescent proteins under the promoters of interneuron-specific markers, provides an efficient method to target and electrophysiologically characterize intrinsic and synaptic properties of specific interneuron types. Combined with intracellular dye labeling, this approach can be extended with post-hoc morphological and immunocytochemical analysis, enabling systematic identification of recorded neurons. These methods can be tailored to suit a broad range of scientific questions regarding functional properties of diverse types of cortical neurons.

Cortical networks are controlled by a small, but diverse set of inhibitory interneurons. Functional investigation of interneurons therefore requires targeted recording and rigorous identification. Described here is a combined approach involving whole-cell recordings from single or synaptically-coupled pairs of neurons with intracellular labeling, post-hoc morphological and immunocytochemical analysis.

GABAergic inhibitory interneurons play a central role within neuronal circuits of the brain. Interneurons comprise a small subset of the neuronal ...

Whole-cell Patch-clamp Recordings in Brain Slices

Whole-cell patch-clamp recording is an electrophysiological technique that allows the study of the&#160;electrical properties of a substantial part of the neuron. In this configuration, the micropipette is in tight contact with the cell membrane, which prevents current leakage and thereby provides more accurate ionic current measurements than the previously used intracellular sharp electrode recording method. Classically, whole-cell recording can be performed on neurons in various types of preparations, including cell culture models, dissociated neurons, neurons in brain slices, and in intact anesthetized or awake animals. In summary, this technique has immensely contributed to the understanding of passive and active biophysical properties of excitable cells. A major advantage of this technique is that it provides information on how specific manipulations (e.g., pharmacological, experimenter-induced plasticity) may alter specific neuronal functions or channels in real-time. Additionally, significant opening of the plasma membrane allows the internal pipette solution to freely diffuse into the cytoplasm, providing means for introducing drugs, e.g., agonists or antagonists of specific intracellular proteins, and manipulating these targets without altering their functions in neighboring cells. This article will focus on whole-cell recording performed on neurons in brain slices,&#160;a preparation that has the advantage of recording neurons in relatively well preserved brain circuits, i.e., in a physiologically relevant context. In particular,&#160;when combined with appropriate pharmacology, this technique is a powerful tool allowing identification of specific neuroadaptations that occurred following any type of experiences, such as learning, exposure to drugs of abuse, and stress. In summary, whole-cell patch-clamp recordings in brain slices provide means to measure in ex vivo preparation long-lasting changes in neuronal functions that have developed in intact awake animals.

This protocol describes basic procedural steps for performing whole-cell patch-clamp recordings. This technique allows the study of&#160;the electrical behavior of neurons, and when performed in brain slices, allows the assessment of various neuronal functions from neurons that are still integrated in relatively well preserved brain circuits.

Whole-cell patch-clamp recording is an electrophysiological technique that allows the study of the&#160;electrical properties of a substantial part of the ...

Subcellular Patch-clamp Recordings from the Somatodendritic Domain of Nigral Dopamine Neurons

Dendrites of dopaminergic neurons receive and convey synaptic input, support action potential back-propagation and neurotransmitter release. Understanding these fundamental functions will shed light on the information transfer in these neurons. Dendritic patch-clamp recordings provide the possibility to directly examine the electrical properties of dendrites and underlying voltage-gated ion channels. However, these fine structures are not easily accessible to patch pipettes because of their small diameter. This report describes a step-by-step procedure to collect stable and reliable recordings from the dendrites of dopaminergic neurons in acute slices. Electrophysiological measurements are combined with post hoc recovery of cell morphology. Successful experiments rely on improved preparation of slices, solutions and pipettes, adequate adjustment of the optics and stability of the pipette in contact with the recorded structure. Standard principles of somatic patch-clamp recording are applied to dendrites but with a gentler approach of the pipette. These versatile techniques can be implemented to address various questions concerning the excitable properties of dendrites.

Subcellular patch-clamp recordings offer the possibility to investigate the functional properties of dendrites. However these fine structures are not easily accessible due to their small diameter. The protocol described here aims to facilitate the collection of stable and reliable recordings from the dendrites of dopamine neurons in slices in vitro.

Dendrites of dopaminergic neurons receive and convey synaptic input, support action potential back-propagation and neurotransmitter release. Understanding ...

Whole-cell Patch-clamp Recordings for Electrophysiological Determination of Ion Selectivity in Channelrhodopsins

Over the past decade, channelrhodopsins became indispensable in neuroscientific research where they are used as tools to non-invasively manipulate electrical processes in target cells. In this context, ion selectivity of a channelrhodopsin is of particular importance. This article describes the investigation of chloride selectivity for a recently identified anion-conducting channelrhodopsin of Proteomonas sulcata via electrophysiological patch-clamp recordings on HEK293 cells. The experimental procedure for measuring light-gated photocurrents demands a fast switchable &#8211; ideally monochromatic &#8211; light source coupled into the microscope of an otherwise conventional patch-clamp setup. Preparative procedures prior to the experiment are outlined involving preparation of buffered solutions, considerations on liquid junction potentials, seeding and transfection of cells, and pulling of patch pipettes. The actual recording of current-voltage relations to determine the reversal potentials for different chloride concentrations takes place 24 h to 48 h after transfection. Finally, electrophysiological data are analyzed with respect to theoretical considerations of chloride conduction.

This article describes how the ion selectivity of channelrhodopsin is determined with electrophysiological whole-cell patch-clamp recordings using HEK293 cells. Here, the experimental procedure for investigating chloride selectivity of an anion-selective channelrhodopsin is demonstrated. However, the procedure is transferable to other channelrhodopsins of distinct selectivity.

Over the past decade, channelrhodopsins became indispensable in neuroscientific research where they are used as tools to non-invasively manipulate ...

Preparations and Protocols for Whole Cell Patch Clamp Recording of Xenopus laevis Tectal Neurons

The Xenopus tadpole retinotectal circuit, comprised of the retinal ganglion cells (RGCs) in the eye which form synapses directly onto neurons in the optic tectum, is a popular model to study how neural circuits self-assemble. The ability to carry out whole cell patch clamp recordings from tectal neurons and to record RGC-evoked responses, either in vivo or using a whole brain preparation, has generated a large body of high-resolution data about the mechanisms underlying normal, and abnormal, circuit formation and function. Here we describe how to perform the in vivo preparation, the original whole brain preparation, and a more recently developed horizontal brain slice preparation for obtaining whole cell patch clamp recordings from tectal neurons. Each preparation has unique experimental advantages. The in vivo preparation enables the recording of the direct response of tectal neurons to visual stimuli projected onto the eye. The whole brain preparation allows for the RGC axons to be activated in a highly controlled manner, and the horizontal brain slice preparation allows recording from across all layers of the tectum.

Preparations and Protocols for Whole Cell Patch Clamp Recording of Xenopus laevis Tectal Neurons

In this paper, we discuss three brain preparations used for whole cell patch clamp recording to study the retinotectal circuit of Xenopus laevis tadpoles. Each preparation, with its own specific advantages, contributes to the experimental tractability of the Xenopus tadpole as a model to study neural circuit function.

The Xenopus tadpole retinotectal circuit, comprised of the retinal ganglion cells (RGCs) in the eye which form synapses directly onto neurons in the optic ...

Preparation of Acute Spinal Cord Slices for Whole-cell Patch-clamp Recording in Substantia Gelatinosa Neurons

Recent whole-cell patch-clamp studies from substantia gelatinosa (SG) neurons have provided a large body of information about the spinal mechanisms underlying sensory transmission, nociceptive regulation, and chronic pain or itch development. Implementations of electrophysiological recordings together with morphological studies based on the utility of acute spinal cord slices have further improved our understanding of neuronal properties and the composition of local circuitry in SG. Here, we present a detailed and practical guide for the preparation of spinal cord slices and show representative whole-cell recording and morphological results. This protocol permits ideal neuronal preservation and can mimic in vivo conditions to a certain extent. In summary, the ability to obtain an in vitro preparation of spinal cord slices enables stable current- and voltage-clamp recordings and could thus facilitate detailed investigations into the intrinsic membrane properties, local circuitry and neuronal structure using diverse experimental approaches.

Here, we describe the essential steps for whole-cell patch-clamp recordings made from substantia gelatinosa (SG) neurons in the in vitro spinal cord slice. This method allows the intrinsic membrane properties, synaptic transmission and morphological characterization of SG neurons to be studied.

Recent whole-cell patch-clamp studies from substantia gelatinosa (SG) neurons have provided a large body of information about the spinal mechanisms ...