Name: single sensillum recordings for locust palp sensilla basiconica
Uploaded: 2018-06-23T15:00:00
Description: Watch this Scientific Journal Video about Single Sensillum Recordings for Locust Palp Sensilla Basiconica at JoVE.com

This work is supported by a grant from the National Natural Science Foundation of China (No.31472037). Any mention of trade names or commercial products in this article is solely for the purpose of providing specific information and does not imply a recommendation.

1. Preparation of Instruments and Insect
<ol>
	<li>Preparing tungsten electrodes and stimuli solutions
	<ol>
		<li>Fix a new tungsten wire (diameter of 0.125 mm, length of 75 mm) into a micromanipulator and sharpen it in a 10% (w/v) sodium nitrite (NaNO2) solution in a syringe at 10 V provided by a power supply for about 1 min under a stereomicroscope (40X magnification).</li>
		<li>Dip the sharpened tungsten wire repeatedly into the 10% NaNO2 solution, about 4 mm at 5 V in &#60; ...

<ol>
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R., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Cuticular+hydrocarbon+pheromones+for+social+behavior+and+their+coding+in+the+ant+antenna.">Cuticular hydrocarbon pheromones for social behavior and their coding in the ant antenna.</a> Cell Reports. 12 (8), 1261-1271 (2015).</li><li>de Bruyne, M., Clyne, P. J., Carlson, J. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Odor+coding+in+a+model+olfactory+organ:+the+Drosophila+maxillary+palp.">Odor coding in a model olfactory organ: the Drosophila maxillary palp.</a> Journal of Neuroscience. 19 (11), 4520-4532 (1999).</li><li>Syed, Z., Leal, W. S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Maxillary+palps+are+broad+spectrum+odorant+detectors+in+Culex+quinquefasciatus.">Maxillary palps are broad spectrum odorant detectors in Culex quinquefasciatus.</a> Chemical Senses. 32 (8), 727-738 (2007).</li><li>Lu, T., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Odor+coding+in+the+maxillary+palp+of+the+malaria+vector+mosquito+Anopheles+gambiae.">Odor coding in the maxillary palp of the malaria vector mosquito Anopheles gambiae.</a> Current Biology. 17 (18), 1533-1544 (2007).</li><li>Pellegrino, M., Nakagawa, T., Vosshall, L. B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Single+sensillum+recordings+in+the+insects+Drosophila+melanogaster+and+Anopheles+gambiae.">Single sensillum recordings in the insects Drosophila melanogaster and Anopheles gambiae.</a> Journal of Visualized Experiments. 36, e1725 (2010).</li><li>Grant, A. J., Wigton, B. E., Aghajanian, J. G., O'Connell, R. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Electrophysiological+responses+of+receptor+neurons+in+mosquito+maxillary+palp+sensilla+to+carbon+dioxide.">Electrophysiological responses of receptor neurons in mosquito maxillary palp sensilla to carbon dioxide.</a> Journal of Comparative Physiology A. 177 (4), 389-396 (1995).</li><li>Blaney, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+ultrastructure+of+an+olfactory+sensillum+on+the+maxillary+palps+of+Locusta+migratoria+(L.).">The ultrastructure of an olfactory sensillum on the maxillary palps of Locusta migratoria (L.).</a> Cell and Tissue Research. 184 (3), 397-409 (1977).</li><li>Hassanali, A., Njagi, P. G. N., Bashir, M. O. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Chemical+ecology+of+locusts+and+related+acridids.">Chemical ecology of locusts and related acridids.</a> Annual Review of Entomology. 50, 223-245 (2005).</li><li>Chapman, R. F. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Contact+chemoreception+in+feeding+by+phytophagous+insects.">Contact chemoreception in feeding by phytophagous insects.</a> Annual Review of Entomology. 48, 455-484 (2003).</li><li>Chapman, R. F., Sword, G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+importance+of+palpation+in+food+selection+by+a+polyphagous+grasshopper+(Orthoptera:+Acrididae).">The importance of palpation in food selection by a polyphagous grasshopper (Orthoptera: Acrididae).</a> Journal of Insect Behavior. 6, 79-91 (1993).</li><li>Winstanley, C., Blaney, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Chemosensory+mechanisms+of+locusts+in+relation+to+feeding.">Chemosensory mechanisms of locusts in relation to feeding.</a> Entomologia Experimentalis et Applicata. 24, 750-758 (1978).</li><li>Blaney, W., Duckett, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+significance+of+palpation+by+the+maxillary+palps+of+Locusta+migratoria+(L.):+an+electrophysiological+and+behavioural+study.">The significance of palpation by the maxillary palps of Locusta migratoria (L.): an electrophysiological and behavioural study.</a> Journal of Experimental Biology. 63, 701-712 (1975).</li><li>Blaney, W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Electrophysiological+responses+of+the+terminal+sensilla+on+the+maxillary+palps+of+Locusta+migratoria+(L.)+to+some+electrolytes+and+non-electrolytes.">Electrophysiological responses of the terminal sensilla on the maxillary palps of Locusta migratoria (L.) to some electrolytes and non-electrolytes.</a> Journal of Experimental Biology. 60, 275-293 (1974).</li><li>Jin, X., Zhang, S., Zhang, L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Expression+of+odorant-binding+and+chemosensory+proteins+and+spatial+map+of+chemosensilla+on+labial+palps+of+Locusta+migratoria+(Orthoptera:+Acrididae).">Expression of odorant-binding and chemosensory proteins and spatial map of chemosensilla on labial palps of Locusta migratoria (Orthoptera: Acrididae).</a> Anthropod Structure &amp; Development. 35 (1), 47-56 (2006).</li><li>Zhang, L., Li, H., Zhang, L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Two+olfactory+pathways+to+detect+aldehydes+on+locust+mouthpart.">Two olfactory pathways to detect aldehydes on locust mouthpart.</a> International Journal of Biological Sciences. 13 (6), 759-771 (2017).</li><li>Dweck, H. K. M., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Olfactory+channels+associated+with+the+Drosophila+maxillary+palp+mediate+short-+and+long-range+attraction.">Olfactory channels associated with the Drosophila maxillary palp mediate short- and long-range attraction.</a> eLife. 5, e14925 (2016).</li><li>Bohbot, J. D., Sparks, J. T., Dickens, J. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=The+maxillary+palp+of+Aedes+aegypti,+a+model+of+multisensory+Integration.">The maxillary palp of Aedes aegypti, a model of multisensory Integration.</a> Insect Biochemistry and Molecular Biology. 48, 29-39 (2014).</li><li>Delventhal, R., Kiely, A., Carlson, J. 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S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Electrophysiological+measurements+from+a+moth+olfactory+system.">Electrophysiological measurements from a moth olfactory system.</a> Journal of Visualized Experiments. 49, e2489 (2011).</li><li>Saha, D., Leong, K., Katta, N., Raman, B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Multi-unit+recording+methods+to+characterize+neural+activity+in+the+locust+(Schistocerca+Americana)+olfactory+circuits.">Multi-unit recording methods to characterize neural activity in the locust (Schistocerca Americana) olfactory circuits.</a> Journal of Visualized Experiments. 71, e50139 (2013).</li><li>Liu, F., Liu, N. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Using+single+sensillum+recording+to+detect+olfactory+neuron+responses+of+bed+bugs+to+semiochemicals.">Using single sensillum recording to detect olfactory neuron responses of bed bugs to semiochemicals.</a> Journal of Visualized Experiments. 107, e53337 (2016).</li></ol>

Insects rely on palps to detect food odors, and their palps are believed to play an important role in speciation13,27. The palps are simple olfactory organs and are receiving increasing attention as an attractive model for the exploration of the neuromolecular networks underlying chemosensation28.
Insect labellar and palp SSRs have been successfully performed on Drosophila melanogaster, Anopheles ga...

Animals have evolved a range of chemosensory organs that sense exogenous chemical cues. In insects, the most important chemosensory organs are the antennae and the palps. On these organs, several types of chemosensory hairs, called chemosensory sensilla, are innervated by chemosensory neurons (CSNs) within the hairs. CSNs in chemosensory sensilla recognize specific chemical cues through signal transduction from chemical stimuli to electrical potentials that are subsequently transferred up to the central nervous systems1,2,3.
CSNs express various chemosensory receptors [e.g., odorant receptors (ORs)], ionotropic receptors (IRs), and gustatory receptors (GRs) on their membranes, which encode exogenous chemical cues associated with different types of chemosensation4,5,6. The characterization of CSNs is key to the elucidation of cellular and molecular mechanisms of insect chemoreception. Now single sensillum recording (SSR) is a widely-used technique for the characterization of insect CSNs in the antennal sensilla of many insects, including flies7, moths8, beetles9, aphids10, locusts11, and ants12. However, few studies have applied an SSR to insect palps13,14,15,16,17, because the particular structures of their sensilla make an electrophysiological recording difficult18.
Swarms of locusts (Orthoptera) often cause serious crop damage and economic loss19. The palps are believed to play an important role in the food selection of locusts20,21,22,23,24. Two types of chemosensory sensilla are investigated by a scanning electron microscope (SEM). Usually, 350 sensilla chaetica and 7 - 8 sensilla basiconica are observed on each dome of the locust palps18. Sensilla chaetica are gustatory sensilla that sense non-volatile chemical cues, whereas sensilla basiconica have an olfactory function, sensing volatile chemical cues.
On locust palps, the diameters of the hair sockets of the sensilla basiconica (ca. 12 &#181;m), are much greater than those of sensilla chaetica (ca. 8 &#181;m)18,25. The cuticular wall of the sensilla basiconica on the palps is much thicker than that of antennal sensilla18. In addition, the dome of the palp has fluid contents within a highly flexible cuticle. These characteristics mean that a penetration with a microelectrode and an acquisition of good electrophysiological signals is more difficult than for antennal sensilla. In this paper, a detailed and highly effective SSR protocol for locust palp sensilla basiconica is presented with a video.

<table border="0" cellpadding="0" cellspacing="0" style="width:1145px;" width="1145">
	<tbody>
		<tr height="40">
			<td height="40" style="height:40px;width:303px;">Tungsten wire</td>
			<td style="width:140px;">ADVENT</td>
			<td style="width:217px;">W559504</td>
			<td style="width:485px;">Used for making the electrode and fixing the palp</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">NaNO2</td>
			<td>Sigma-aldrich</td>
			<td>563218-25G</td>
			<td>Used for sharpening the tungsten wire</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">AC Power Supply</td>
			<td>Syntech</td>
			<td>A2-70</td>
			<td>Providing the voltage in sharpening the tungsten wire</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Stereoscope</td>
			<td>Motic</td>
			<td>SMZ-163</td>
			<td>Used for observing the sharpening of tungsten wire</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Microscope</td>
			<td>Olympus</td>
			<td>W-51</td>
			<td>Used for observing the sensilla on locust maxillary palp</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Intelligent Data Acquisition Controller</td>
			<td>Syntech</td>
			<td>IDAC-4</td>
			<td>Real-time on screen display of all signals before and during recording</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Stimulus controller</td>
			<td>Syntech</td>
			<td>CS-55</td>
			<td>Used for controlling the stimulus application</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Electronic micromanipulator</td>
			<td>C.M.D.T</td>
			<td>CFT-8301D</td>
			<td>Used for minor movement of the recording electrode</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Micromanipulator</td>
			<td>Narishige</td>
			<td>MN-151</td>
			<td>Used for minor movement of the reference electrode</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Speaker</td>
			<td>EDIFIER</td>
			<td>R101T06</td>
			<td>Connected with IDAC-4 and providing sound for the signal</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Magnetic base</td>
			<td>PDOK</td>
			<td>PD-101</td>
			<td>Used to hold the electrode, and stimulus delivery tube</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Vibration Isolation Table</td>
			<td>TianHe</td>
			<td>HAP-100-1208</td>
			<td>Used for isolating the vibration from the equipment</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Glass slide</td>
			<td>CITOGLAS</td>
			<td>ZBP-407</td>
			<td>Used for making the base for the MPH</td>
		</tr>
		<tr height="40">
			<td height="40" style="height:40px;">Blu-tack</td>
			<td>Bostik</td>
			<td>Blu-tack-45g</td>
			<td>Fixing the tungsten wire</td>
		</tr>
		<tr height="32">
			<td height="32" style="height:32px;">Pasteur tube</td>
			<td>YARE</td>
			<td>WITEG</td>
			<td>Placing the filter paper containing stimuli solutions</td>
		</tr>
	</tbody>
</table>

single sensillum recordings for locust palp sensilla basiconica

The palps of locust mouthparts are considered to be conventional gustatory organs that play an important role in a locust&#39;s food selection, especially for the detection of non-volatile chemical cues through sensilla chaetica (previously named terminal sensilla or crested sensilla). There is now increasing evidence that these palps also have an olfactory function. An odorant receptor (LmigOR2) and an odorant-binding protein (LmigOBP1) have been localized in the neurons and accessory cells, respectively, in the sensilla basiconica of the palps. Single sensillum recording (SSR) is used for recording the responses of odorant receptor neurons, which is an effective method for screening active ligands on specific odorant receptors. SSR is used in functional studies of odorant receptors in palp sensilla. The structure of the sensilla basiconica located on the dome of the palps differs somewhat from the structure of those on the antennae. Therefore, when performing an SSR elicited by odorants, some specific advice may be helpful for obtaining optimum results. In this paper, a detailed and highly effective protocol for an SSR from insect palp sensilla basiconica is introduced.

Two sensilla subtypes (pb1 and pb2) on the locust maxillary palp are identified based on different response dynamics to chemical odorants (10% 1-nonanol and 10% nonanoic acid). The neurons in pb1 produce significantly more spikes to 1-nonanol than to nonanoic acid while the neurons in pb2 are significantly less activated by 1-nonanol compared with nonanoic acid (Figure 4). Hexanal and E-2-Hexenal can evoke a locust palp opening response (POR)<sup class="xref"...

Watch this Scientific Journal Video about Single Sensillum Recordings for Locust Palp Sensilla Basiconica at JoVE.com

Single Sensillum Recordings for Locust Palp Sensilla Basiconica

This paper describes a detailed and highly effective protocol for single sensillum recordings from the sensilla basiconica on the palps of insect mouthparts.

The palps of locust mouthparts are considered to be conventional gustatory organs that play an important role in a locust&#39;s food selection, especially ...

The overall goal of this procedure is to introduce a detailed and highly effective protocol to make single sensillum recordings from insect palp Sensilla Basiconica. Since mastered can help answer key questions in the dissection chemoreception field. By allowing of specific odorant receptor in palp sensilla.The main advantage of this is that use a recorder Sensilla Basiconia of locust of the palps. To prepare the tungsten electrodes first attach a new tungsten wire into a micro manipulator and observe it under 40 times magnification. Now sharpen the wire by delivering 10 volts to it while using a syringe to apply 10%sodium nitrite.Then reduce the power to five volts and over one minute repeatedly dip four millimeters of the sharpened wire into sodium nitrite solution. When in use the tip must be fine enough to penetrate the cuticle of a locust palp olfactory sensillum. Next prepare the stimulus solutions.Dilute each of the chemical stimulus substances in mineral oil. Make 10%dilutions of 1-Nonanol and Nonanoic acid in mineral oil. Then make a series of tenfold serial dilutions of E-2-Hexenal and Hexanal in mineral oil.Next prepare Pasteur tubes loaded with stimuli. Insert filter paper strips into the tubes and add 10 microliters of the diluted stimulus solutions to the filter paper strips. Then plug the tubes with one milliliter pipette tips.From the recordings make a locust maxillary palp holder from a glass slide, a piece of plastic, a cover slip and double sided tape and rubber tape. Attach the plastic piece to a corner of the slide using double sided tape and then use another piece of tape to attach the cover slip to the plastic piece. Then attach a small piece of red rubber tape onto the cover glass to make it a non-slip surface.Next using the tape attach a tungsten wire 1.5 millimeters parallel to the inside edge of the platform and fix both ends of the wire onto the platform. This completes the holder. Rear the locust on fresh wheat seedlings and at 60%humidity 28 to 30 degrees Celsius and with an 18 hour light cycle.To collect the antenna select one day to three day old fifth instar Locust nymphs. Remove the antenna using fine scissors so they cannot interfere with the recording. To secure the locust use a 1.5 millimeter tube cut in 1/2 vertically.Leave the ventral region and the head of the locust exposed. Then fix the locust and tube to the glass slide with double sided adhesive tape. Next pull the right maxillary palp out and position it onto the platform.Put the tungsten wire at the fourth segment of the palp. Now surround the tungsten wire with blue Taft putty about two millimeters from the maxillary palp. It is critical to the to most properly set up the platform with a centimeter locust maxillary palp holder and to use the tungsten wire to comprise the four segment or the palp.Now view the preparation at 100%times magnification and position the palp perpendicularly to the recording electrode. Next using a micromanipulator insert a tungsten reference electrode into the locust eye. Then move the recording electrode close to the maxillary palp.Next position the odor delivery device about one centimeter from the maxillary palp. Now open the recording software and set the recording parameters. For the recording scale use 500 microvolts.For the high cut off of the filter use 300 hertz. Set the low cutoff to 200 hertz and set the pre-trigger to 10 seconds. Now switch the microscope to a high magnification and insert the recording electrode into the base of a basiconic sensillum on the maxillary palp.Then delicately adjust the recording electrode to obtain good spontaneous spikes. It is very important that the recording electrode penetrates into the base of the sensillum and that once into the sensillum are prepared. Now open the stimulus controller to deliver a continuous airstream at 20 millimeters per second.Next set the stimulation time to one second and record signals for 10 seconds starting 10 seconds before the onset of the stimulus pulse. Now collect the data. Two sensilla subtypes on the locust maxillary palp were distinguishable based on their response dynamics to the chemical stimulants 1-Nonanol and Nonanoic acid.The odorants Hexanal and E-2-Hexanal naturally occurring in food sources can evoke a locust palp opening response. In response E-2-Hexanal pb1 neurons have longer action potentials. Comparing the mean changes in spiking during the five seconds before stimulation to the five seconds after stimulation shows that the response to 1-Nonanol is significantly higher than Nonanoic acid in the pb1 neurons.And the reverse is true for pb2 neurons. The response by these neurons to E-2-Hexenal and hexanal is also dose dependent. The two neuron types have a different dose response pattern to E-2-Hexenal, but the response to hexanal is mostly the same.After watching this video you should have a good understanding of how to perform the highly effective single sensilla recording on locust palp Sensilla Basonica. Once mastered the technique can be done if it is performed properly. When attempting this procedure it's important the tube of the palp from when the recording electrode is inserted into the base of sensillum.After this development paved the way for research in the field of insect physiology to the and cellular mechanisms of incellular olfaction in the mouth part.

single-sensillum-recordings-for-locust-palp-sensilla-basiconica

Research

JoVE Journal

Neuroscience

Single Sensillum Recordings in the Insects Drosophila melanogaster and Anopheles gambiae

The sense of smell is essential for insects to find foods, mates, predators, and oviposition sites3. Insect olfactory sensory neurons (OSNs) are enclosed in sensory hairs called sensilla, which cover the surface of olfactory organs. The surface of each sensillum is covered with tiny pores, through which odorants pass and dissolve in a fluid called sensillum lymph, which bathes the sensory dendrites of the OSNs housed in a given sensillum. The OSN dendrites express odorant receptor (OR) proteins, which in insects function as odor-gated ion channels4, 5. The interaction of odorants with ORs either increases or decreases the basal firing rate of the OSN. This neuronal activity in the form of action potentials embodies the first representation of the quality, intensity, and temporal characteristics of the odorant6, 7.
Given the easy access to these sensory hairs, it is possible to perform extracellular recordings from single OSNs by introducing a recording electrode into the sensillum lymph, while the reference electrode is placed in the lymph of the eye or body of the insect. In Drosophila, sensilla house between one and four OSNs, but each OSN typically displays a characteristic spike amplitude. Spike sorting techniques make it possible to assign spiking responses to individual OSNs. This single sensillum recording (SSR) technique monitors the difference in potential between the sensillum lymph and the reference electrode as electrical spikes that are generated by the receptor activity on OSNs1, 2, 8. Changes in the number of spikes in response to the odorant represent the cellular basis of odor coding in insects. Here, we describe the preparation method currently used in our lab to perform SSR on Drosophila melanogaster and Anopheles gambiae, and show representative traces induced by the odorants in a sensillum-specific manner.

Single Sensillum Recordings in the Insects Drosophila melanogaster and Anopheles gambiae

Electrophysiological responses of olfactory sensory neurons to odorants can be measured in insects using single sensillum recordings. In this video article we will demonstrate how to perform single sensillum recordings in the antennae of the vinegar fly (Drosophila melanogaster) and the maxillary palps of the malaria mosquito (Anopheles gambiae).

The sense of smell is essential for insects to find foods, mates, predators, and oviposition sites3. Insect olfactory sensory neurons (OSNs) are enclosed ...

Single-unit In vivo Recordings from the Optic Chiasm of Rat

Information about the visual world is transmitted to the brain in sequences of action potentials in retinal ganglion cell axons that make up the optic nerve. In vivo recordings of ganglion cell spike trains in several animal models have revealed much of what is known about how the early visual system processes and encodes visual information. However, such recordings have been rare in one of the most common animal models, the rat, possibly owing to difficulty in detecting spikes fired by small diameter axons. The many retinal disease models involving rats motivate a need for characterizing the functional properties of ganglion cells without disturbing the eye, as with intraocular or in vitro recordings. Here, we demonstrate a method for recording ganglion cell spike trains from the optic chiasm of the anesthetized rat. We first show how to fabricate tungsten-in-glass electrodes that can pick up electrical activity from single ganglion cell axons in rat. The electrodes outperform all commercial ones that we have tried. We then illustrate our custom-designed stereotaxic system for in vivo visual neurophysiology experiments and our procedures for animal preparation and reliable and stable electrode placement in the optic chiasm.

Single-unit In vivo Recordings from the Optic Chiasm of Rat

Retinal ganglion cells transmit visual information from the eye to the brain with sequences of action potentials. Here, we demonstrate how to record the action potentials of single ganglion cells in vivo from anesthetized rats.

Information about the visual world is transmitted to the brain in sequences of action potentials in retinal ganglion cell axons that make up the optic ...

Electrophysiology of Scorpion Peg Sensilla

We describe a modification of an existing tip-recording technique1,2 for electrophysiologically investigating short, peg-like sensory sensilla3,4. On the mid-ventral surface of all scorpions are two appendages called pectines, which have dense fields of mechano- and chemosensory peg sensilla5,6. One method for assessing chemoresponsiveness of these sensilla uses a tungsten electrode for extracellularly recording neural activity within a sensillum as a volatile odorant is introduced to the sensory field5,7. The limitations of this method include slow data collection and uncontrolled stimulant introduction to, and removal from, the peg field. To overcome these limitations, we developed a new tip-recording technique that uses nonpolar mineral oil as a medium through which to deliver water-based tastants to individual peg sensilla8,9. We have successfully applied this method to obtain sensillar chemoresponses to citric acid, ethanol, and salt. Here we describe the experimental protocol for such a study9. We think this new method may be useful for studying the response properties of other arthropod chemosensory systems, including those of insects10, 11 and crustaceans12.

This article describes an electrophysiological method for isolating chemical stimulation to individual sensilla via extracellular, tip-recordings under mineral oil.

We describe a modification of an existing tip-recording technique1,2 for electrophysiologically investigating short, peg-like sensory sensilla3,4. On the ...

A Procedure for Implanting Organized Arrays of Microwires for Single-unit Recordings in Awake, Behaving Animals

In vivo electrophysiological recordings in the awake, behaving animal provide a powerful method for understanding neural signaling at the single-cell level. The technique allows experimenters to examine temporally and regionally specific firing patterns in order to correlate recorded action potentials with ongoing behavior. Moreover, single-unit recordings can be combined with a plethora of other techniques in order to produce comprehensive explanations of neural function. In this article, we describe the anesthesia and preparation for microwire implantation. Subsequently, we enumerate the necessary equipment and surgical steps to accurately insert a microwire array into a target structure. Lastly, we briefly describe the equipment used to record from each individual electrode in the array. The fixed microwire arrays described are well-suited for chronic implantation and allow for longitudinal recordings of neural data in almost any behavioral preparation. We discuss tracing electrode tracks to triangulate microwire positions as well as ways to combine microwire implantation with immunohistochemical techniques in order to increase the anatomical specificity of recorded results.

Implanting organized arrays of microwires for use in single-unit electrophysiological recordings presents a number of technical challenges.&#160;Methods for performing this technique and the equipment necessary are described.&#160;Also, the beneficial use of organized microwire arrays to record from distinct neural subregions with high spatial selectivity is discussed.

In vivo electrophysiological recordings in the awake, behaving animal provide a powerful method for understanding neural signaling at the single-cell ...

Electrophysiological Recording From Drosophila Labellar Taste Sensilla

The peripheral taste response of insects can be powerfully investigated with electrophysiological techniques. The method described here allows the researcher to measure gustatory responses directly and quantitatively, reflecting the sensory input that the insect nervous system receives from taste stimuli in its environment. This protocol outlines all key steps in performing this technique. The critical steps in assembling an electrophysiology rig, such as selection of necessary equipment and a suitable environment for recording, are delineated. We also describe how to prepare for recording by making appropriate reference and recording electrodes, and tastant solutions. We describe in detail the method used for preparing the insect by insertion of a glass reference electrode into the fly in order to immobilize the proboscis. We show traces of the electrical impulses fired by taste neurons in response to a sugar and a bitter compound. Aspects of the protocol are technically challenging and we include an extensive description of some common technical challenges that may be encountered, such as lack of signal or excessive noise in the system, and potential solutions. The technique has limitations, such as the inability to deliver temporally complex stimuli, observe background firing immediately prior to stimulus delivery, or use water-insoluble taste compounds conveniently. Despite these limitations, this technique (including minor variations referenced in the protocol) is a standard, broadly accepted procedure for recording Drosophila neuronal responses to taste compounds.

Electrophysiological Recording From Drosophila Labellar Taste Sensilla

This protocol describes extracellular recording of the action potential responses fired by labellar taste neurons in Drosophila.

The peripheral taste response of insects can be powerfully investigated with electrophysiological techniques. The method described here allows the ...

Paired Whole Cell Recordings in Organotypic Hippocampal Slices

Pair recordings involve simultaneous whole cell patch clamp recordings from two synaptically connected neurons, enabling not only direct electrophysiological characterization of the synaptic connections between individual neurons, but also pharmacological manipulation of either the presynaptic or the postsynaptic neuron. When carried out in organotypic hippocampal slice cultures, the probability that two neurons are synaptically connected is significantly increased. This preparation readily enables identification of cell types, and the neurons maintain their morphology and properties of synaptic function similar to that in native brain tissue. A major advantage of paired whole cell recordings is the highly precise information it can provide on the properties of synaptic transmission and plasticity that are not possible with other more crude techniques utilizing extracellular axonal stimulation. Paired whole cell recordings are often perceived as too challenging to perform. While there are challenging aspects to this technique, paired recordings can be performed by anyone trained in whole cell patch clamping provided specific hardware and methodological criteria are followed. The probability of attaining synaptically connected paired recordings significantly increases with healthy organotypic slices and stable micromanipulation allowing independent attainment of pre- and postsynaptic whole cell recordings. While CA3-CA3 pyramidal cell pairs are most widely used in the organotypic slice hippocampal preparation, this technique has also been successful in CA3-CA1 pairs and can be adapted to any neurons that are synaptically connected in the same slice preparation. In this manuscript we provide the detailed methodology and requirements for establishing this technique in any laboratory equipped for electrophysiology.

Pair recordings are simultaneous whole cell patch clamp recordings from two synaptically connected neurons, enabling precise electrophysiological and pharmacological characterization of the synapses between individual neurons. Here we describe the detailed methodology and requirements for establishing this technique in organotypic hippocampal slice cultures in any laboratory equipped for electrophysiology.

Pair recordings involve simultaneous whole cell patch clamp recordings from two synaptically connected neurons, enabling not only direct ...

Using Single Sensillum Recording to Detect Olfactory Neuron Responses of Bed Bugs to Semiochemicals

The insect olfactory system plays an important role in detecting semiochemicals in the environment. In particular, the antennal sensilla which house single or multiple neurons inside, are considered to make the major contribution in responding to the chemical stimuli. By directly recording action potential in the olfactory sensillum after exposure to stimuli, single sensillum recording (SSR) technique provides a powerful approach for investigating the neural responses of insects to chemical stimuli. For the bed bug, which is a notorious human parasite, multiple types of olfactory sensillum have been characterized. In this study, we demonstrated neural responses of bed bug olfactory sensilla to two chemical stimuli and the dose-dependent responses to one of them using the SSR method. This approach enables researchers to conduct early screening for individual chemical stimuli on the bed bug olfactory sensilla, which would provide valuable information for the development of new bed bug attractants or repellents and benefits the bed bug control efforts.

Bed bugs rely on olfactory receptor neurons housed in their antennal olfactory sensilla to detect semiochemicals in the environment. Utilizing single sensillum recording, we demonstrate a method to evaluate bed bug response to semiochemicals and explore the coding process involved.

The insect olfactory system plays an important role in detecting semiochemicals in the environment. In particular, the antennal sensilla which house ...

Localization of Odorant Receptor Genes in Locust Antennae by RNA In Situ Hybridization

Insects have evolved sophisticated olfactory reception systems to sense exogenous chemical signals. These chemical signals are transduced by Olfactory Receptor Neurons (ORNs) housed in hair-like structures, called chemosensilla, of the antennae. On the ORNs&#39; membranes, Odorant Receptors (ORs) are believed to be involved in odor coding. Thus, being able to identify genes localized to the ORNs is necessary to recognize OR genes, and provides a fundamental basis for further functional in situ studies. The RNA expression levels of specific ORs in insect antennae are very low, and preserving insect tissue for histology is challenging. Thus, it is difficult to localize an OR to a specific type of sensilla using RNA in situ hybridization. In this paper, a detailed and highly effective RNA in situ hybridization protocol particularly for lowly expressed OR genes of insects, is introduced. In addition, a specific OR gene was identified by conducting double-color fluorescent in situ hybridization experiments using a co-expressing receptor gene, Orco, as a marker.

Localization of Odorant Receptor Genes in Locust Antennae by RNA In Situ Hybridization

This paper describes a detailed and highly effective RNA in situ hybridization protocol particularly for low-level expressed Odorant Receptor (OR) genes, as well as other genes, in insect antennae using digoxigenin (DIG)-labeled or biotin-labeled probes.

Insects have evolved sophisticated olfactory reception systems to sense exogenous chemical signals. These chemical signals are transduced by Olfactory ...

Electrophysiological Recording from Drosophila Trichoid Sensilla in Response to Odorants of Low Volatility

Insects rely on their sense of smell to guide a wide range of behaviors that are critical for their survival, such as food-seeking, predator avoidance, oviposition, and mating. Myriad chemicals of varying volatilities have been identified as natural odorants that activate insect Olfactory Receptor Neurons (ORNs). However, studying the olfactory responses to low-volatility odorants has been hampered by an inability to effectively present such stimuli using conventional odor-delivery methods. Here, we describe a procedure that permits the effective presentation of low-volatility odorants for in vivo Single-Sensillum Recording (SSR). By minimizing the distance between the odor source and the target tissue, this method allows for the application of biologically salient but hitherto inaccessible odorants, including palmitoleic acid, a stimulatory pheromone with a demonstrated effect on ORNs involved in courtship and mating behavior1. Our procedure thus affords a new avenue to assay a host of low-volatility odorants for the study of insect olfaction and pheromone communication.

Electrophysiological Recording from Drosophila Trichoid Sensilla in Response to Odorants of Low Volatility

The overall goal of this protocol is to demonstrate how to present odorants of low volatility for single-sensillum recording from Drosophila olfactory receptor neurons that respond to long-chain cuticular pheromones.

Insects rely on their sense of smell to guide a wide range of behaviors that are critical for their survival, such as food-seeking, predator avoidance, ...

Investigating Object Representations in the Macaque Dorsal Visual Stream Using Single-unit Recordings

Previous studies have shown that neurons in parieto-frontal areas of the macaque brain can be highly selective for real-world objects, disparity-defined curved surfaces, and images of real-world objects (with and without disparity) in a similar manner as described in the ventral visual stream. In addition, parieto-frontal areas are believed to convert visual object information into appropriate motor outputs, such as the pre-shaping of the hand during grasping. To better characterize object selectivity in the cortical network involved in visuomotor transformations, we provide a battery of tests intended to analyze the visual object selectivity of neurons in parieto-frontal regions.

A detailed protocol to analyze object selectivity of parieto-frontal neurons involved in visuomotor transformations is presented.

Previous studies have shown that neurons in parieto-frontal areas of the macaque brain can be highly selective for real-world objects, disparity-defined ...