Name: Identification of Olfactory Volatiles using Gas Chromatography-Multi-unit Recordings (GCMR) in the Insect Antennal Lobe (Video) | JoVE Journal
Uploaded: 2013-02-24T14:00:00.000+00:00
Duration: 9 min 49 s
Description: Learn to identify biologically active odorants in complex scents using gas chromatography and multi-unit recordings in the bumblebee antennal lobe. This method enables precise neural characterization of floral volatiles.

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This work was supported by NSF grant IOS 1121692, and by the University of Washington's Research Foundation.

1. Volatile Follection
 <ol>
 <li>In this example, we use volatile samples from M. lewisii flowers - an alpine wildflower native to California. Volatiles are collected using dynamic sorption methods according to Riffell et al.14. Briefly, this method employs a closed loop trapping system where flowers are enclosed in a Teflon bag. Using an inert vacuum pump, the air around the flowers is sucked through a "trap" comprised of a Pasteur pipette filled with Porapak Q matrix. The return air from the pump is filtered by activated charcoal. After a prescribed time period, in our case 24 h, the Porapak Q matrix is eluted with a non-polar solvent, typically hexane, to collect the concentrated extract. The extract is then stored in -80 &deg;C until analysis. If necessary, samples can be concentrated prior to analysis under a stream of nitrogen gas. Unless the sample is already well-characterized, run an aliquot of it through a gas chromatograph-mass spectrometer (GC-MS) to identify volatile components prior to using the sample.</li>
 </ol>
 2. Electrophysiological Preparation
 <ol>
 <li>Cut approximately 1 cm from the end of a 1,000 &mu;l pipette tip. Place a bumble bee (Bombus impatiens) into the base of the pipette tip and gently push towards the opposite end of the tip until only the head is exposed.</li>
 <li>Melt dental wax and mold it around the exposed head, making sure that the wax adheres onto the compound eyes for security and to make the bee's head completely immobile. Be sure not to get any wax onto the antenna of the bee.</li>
 <li>Once the head is secure, make a square, window-like, incision into the head capsule using a razor blade-breaker or the appropriate sized scalpel to cut the cuticle. Using the blade-breaker, start from the dorsal side of the head capsule, immediately behind the antenna and adjacent to one of the compound eyes. Cut a straight line, from one compound eye to the contralateral compound eye. After cutting a straight line to the opposite compound eye, begin making an incision dorsally until the head capsule curves and ends near its thorax. At this point, begin to cut towards the opposite end of the head capsule. Finally, once a line has been cut to the opposite end, cut a line back up to the starting position of the initial incision. It is important to remove the cuticle that is adjacent to the antenna, as this will impede the insertion of the electrode.</li>
 <li>Once the cuticle is cut, use a pair of forceps to remove the bee cuticle, which should then expose the bee's brain and, more importantly, the antennal lobes. Immediately begin superfusing the brain with insect saline, so that the brain does not become dessicated. After the brain is exposed, carefully use a pair of very fine forceps to remove the perineural sheath immediately above the antennal lobes. Be very careful not to puncture the bee's brain with the forceps.</li>
 </ol>
 3. Gas Chromatography with Multi-channel Recording
 <ol>
 <li>The bee "preparation" - fixed in a tube with its brain exposed - is now ready for electrophysiological recording. Place the bee in a clamp, fixed to a magnetic base that is located on an air table.</li>
 <li>Arrange an IV bag, flow controller, and tubing (filled with insect saline) so that the saline continuously superfuses the brain.</li>
 <li>Using a micromanipulator, insertareference electrode, made of tungsten wire, into the bee's eye.</li>
 <li>Using a separate micromanipulator, insert the multi-channel electrode, such as a coiled wire tetrode, or silicon multi-channel electrode (Neuronexus Technologies), into the antennal lobes of the bee. This electrode is connected to a pre-amplifier such as the TDT system's S-3 Z series to the Z-bus bioamp processor of the TDT system. Output from the Gas Chromatogram's detector via a shielded BNC cable can be interfaced with the amplifier and data acquisition system such that both the neural and GC signal is synchronized.</li>
 <li>Wait approximately 30-60 minutes for the neural recordings to stabilize. Once the spontaneous activity and waveform shape of units in the recording channels have become consistent, use an odor syringe to stimulate the bee and observe the response of the recording channels to the odor.</li>
 <li>Record extracellular spikes from neurons by auto-thresholding the recording channels by 3.5 to 5 sigma of the signal on the individual recording channels. Manual thresholding may be required for some channels to avoid contamination from electrical noise. The action potentials from neurons will appear as voltage spikes in the recording channel. When the channel's voltage exceeds the threshold, the system buffers and saves the few milliseconds before and after the crossing of the threshold, thereby taking a snap-shot of the waveform, or spike.</li>
 <li>Immediately next to the air table is the GC. Before injecting the floral extract into the GC, make sure that the method for the temperature ramp of the GC run is correct. In our example, we use a temperature method starting at 50 &deg;C for 4 min followed by an increase of temperature at a rate of 10 &deg;C/min. to 220 &deg;C, at which time we hold the GC for an additional 6 min. We use a DB-5 GC column (J&amp;W Scientific, Folsom, CA, USA), with helium as the carrier gas. The inlet is splitless, with a temperature set to 200 &deg;C. The flame ionization detector temperature is set to 230 &deg;C.</li>
 <li>Inject the extract sample of the floral headspace into the heated injection port of the GC to release the adsorbed volatiles into the GC column. The effluent from the column is split 1:1 between the Flame Ionization Detector (FID) and the bee antenna using a glass "Y" connector (J&amp;W Scientific). Begin recording from the electrode as you inject a sample into the GC.</li>
 <li>After the GC run has finished, let the preparation rest for 5 to 15 min. Then either inject another sample into the GC or stimulate the preparation using single volatile compounds or mixtures of compounds. In this latter method of stimulating the preparation, pulses of air from a constant air stream are diverted through a glass syringe containing a piece of filter paper on which the compounds have been deposited. The odor stimulus was pulsed by means of a solenoid-activated valve controlled by the software.</li>
 <li>If unit activity suddenly stops or changes, check the saline drip and let the preparation rest for 15 min. If the spontaneous activity does not regain its previous level then the preparation should be discarded and another bee used if available.</li>
 <li>After the experiment, fix the brain with 5% formalin for 20 min with the probe still in the tissue. Next, excise the brain and place it in 2% glutaraldehyde for 4 hr, and subsequently do a graded ethanol dehydration series and clear the brain with methyl salicylate. Based on the fixing and clearing of the tissue, the locations in the AL where the electrodes punctured the tissue should be clearly discernible by confocal microscopy.</li>
 </ol>
 4. Data Analysis
 <ol>
 <li>Analyze collected data after the experiment to separate and identify the recorded neural units. Use typical software programs (Offline Sorter, MClust, and SClust) to separate waveforms, or "spikes", based on spike shapes, such as peak or valley amplitude, peak half-width, etc., or reduced measures (principal components)17,18 (Figure 2). Use only those clusters of spikes that separated in three-dimensional space (PC1-PC3) and are statistically different from one another (multivariate ANOVA; p &lt; 0.05) (Figure 2) for further analysis. Please refer to citation #s 17-19 for full description of tetrode recording and spike-sorting methodologies.</li>
 <li>Time-stamp spikes in each cluster, and export these data for analysis using MATLAB or Neuroexplorer (Nex Technologies, Winston-Salem, NC) to create raster plots and firing rate responses (Figures 2, 3A).</li>
 <li>Identify the retention times of volatiles using the simultaneously recorded GC data. Use the retention times of the volatiles, determined by the apex of the peak from the chromatogram, to examine unit responses at those time points.</li>
 <li>To examine individual unit responses through the GC run, bin the number of spikes in 100 msec intervals and examine the time-course of firing rate responses with reference to the retention time of eluting volatiles. The binning of spikes in 100 msec intervals provides enough detail, or signal, about the time-course of the neuronal response to an eluting odorant from the GC.</li>
 <li>To examine the population responses to the different eluting volatiles, integrate the firing rate responses of individual units over a 3 sec sampling window, 1.5 sec before, and 1.5 sec after, the retention time of the volatile (Figure 3). This time period is typical of the duration of an eluting volatile from the GC. We show firing rate responses of the units by color-coding them (red is a high firing rate response; blue is a low response) and arranging them as an activity matrix with each row representing the ensemble response to the GC effluent (columns) (Figure 3).</li>
 </ol>

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<li>Reisenman, C. E., Riffell, J. A., Hildebrand, J. G. International Symposium on Olfaction and Taste. 1170, 462-467 (2009).</li>
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<li>Pellegrino, M., Nakagawa, T., Vosshall, L. B. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Single+sensillum+recordings+in+the+insects+Drosophila+melanogaster+and+Anopheles+gambiae%5BTitle%5D)+AND+%22J+Vis+Exp%22%5BJournal%5D)">Single sensillum recordings in the insects Drosophila melanogaster and Anopheles gambiae.</a> J Vis Exp. (36), e1725(2010).</li>
<li>Syed, Z., Leal, W. S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Electrophysiological+measurements+from+a+moth+olfactory+system%5BTitle%5D)+AND+%22J.+Vis.+Exp%22%5BJournal%5D)">Electrophysiological measurements from a moth olfactory system.</a> J. Vis. Exp. (49), e2489(2011).</li>
<li>Roelofs, W. L., Comeau, A., Hill, A., Milicevic, G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Sex+attractant+of+the+codling+moth%3A+characterization+with+electroantennogram+technique%5BTitle%5D)+AND+%22Science%22%5BJournal%5D)">Sex attractant of the codling moth: characterization with electroantennogram technique.</a> Science. 174, 297-299 (1971).</li>
<li>Riffell, J. A., Lei, H., Christensen, T. A., Hildebrand, J. G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Characterization+and+coding+of+behaviorally+significant+odor+mixtures%5BTitle%5D)+AND+%22Current+Biology%22%5BJournal%5D)">Characterization and coding of behaviorally significant odor mixtures.</a> Current Biology. 19, 335-340 Forthcoming.</li>
<li>Riffell, J. A., Lei, H., Hildebrand, J. G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Neural+correlates+of+behavior+in+the+moth+Manduca+sexta+in+response+to+complex+odors%5BTitle%5D)+AND+%22Proceedings+of+the+National+Academy+of+Sciences+of+the+U.S.A%22%5BJournal%5D)">Neural correlates of behavior in the moth Manduca sexta in response to complex odors.</a> Proceedings of the National Academy of Sciences of the U.S.A. 106, 19219-19226 (2009).</li>
<li>Raguso, R. A., Pellmyr, O. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Dynamic+headspace+analysis+of+floral+volatiles%3A+a+comparison+of+methods%5BTitle%5D)+AND+%22Oikos%22%5BJournal%5D)">Dynamic headspace analysis of floral volatiles: a comparison of methods.</a> Oikos. 81, 238-254 (1998).</li>
<li>Rodriguez-Saona, C. R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Herbivore-induced+blueberry+volatiles+and+intra-plant+signaling%5BTitle%5D)+AND+%22J+Vis+Exp%22%5BJournal%5D)">Herbivore-induced blueberry volatiles and intra-plant signaling.</a> J Vis Exp. , e3440(2011).</li>
<li>Nguyen, D. P., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Micro-drive+array+for+chronic+in+vivo+recording%3A+tetrode+assembly%5BTitle%5D)+AND+%22J+Vis+Exp%22%5BJournal%5D)">Micro-drive array for chronic in vivo recording: tetrode assembly.</a> J Vis Exp. , e1098(2009).</li>
<li>Schjetnan, A. G. P., Luczak, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Recording+large-scale+neuronal+ensembles+with+silicon+probes+in+the+anesthetized+rat%5BTitle%5D)+AND+%22J+Vis+Exp%22%5BJournal%5D)">Recording large-scale neuronal ensembles with silicon probes in the anesthetized rat.</a> J Vis Exp. , e3282(2011).</li>
<li>Deisig, N., Giurfa, M., Lachnit, H., Sandoz, J. -C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Neural+representation+of+olfactory+mixtures+in+the+honeybee+antennal+lobe%5BTitle%5D)+AND+%22European+Journal+of+Neuroscience%22%5BJournal%5D)">Neural representation of olfactory mixtures in the honeybee antennal lobe.</a> European Journal of Neuroscience. 24, 1161-1174 (2006).</li>
<li>Stökl, J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((A+deceptive+pollination+system+targeting+drosophilids+through+olfactory+mimicry+of+yeast%5BTitle%5D)+AND+%22Current+Biology%22%5BJournal%5D)">A deceptive pollination system targeting drosophilids through olfactory mimicry of yeast.</a> Current Biology. 20, 1846-1852 (2010).</li>
<li>Schneider, D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Elektrophysiologische+untersuchungen+von+chemo-+und+mechanorezeptoren+der+antenne+des+seidenspinners+Bombyx+mori+L%5BTitle%5D)+AND+%22Journal+of+Comparative+Physiology+A%3A+Neuroethology%2C+Sensory%2C+Neural%2C+and+Behavioral+Physiology%22%5BJournal%5D)">Elektrophysiologische untersuchungen von chemo- und mechanorezeptoren der antenne des seidenspinners Bombyx mori L.</a> Journal of Comparative Physiology A: Neuroethology, Sensory, Neural, and Behavioral Physiology. 40, 8-41 (1957).</li>
<li>Arn, H., Städler, E., Rauscher, S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((The+electroantennographic+detector%3A+a+selective+and+senstitive+tool+in+the+gas+chromatographic+analysis+of+insect+pheromones%5BTitle%5D)+AND+%22Zeitschrift+f%C3%BCr+Naturforschung%22%5BJournal%5D)">The electroantennographic detector: a selective and senstitive tool in the gas chromatographic analysis of insect pheromones.</a> Zeitschrift für Naturforschung. 30c, 722-725 (1975).</li>
<li>Schneider, D., Boeckh, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Rezeptorpotential+und+nervenimpulse+einzelner+olfaktorischer+sensillen+der+insektenantenne%5BTitle%5D)+AND+%22Journal+of+Comparative+Physiology+A%3A+Neuroethology%2C+Sensory%2C+Neural%2C+and+Behavioral+Physiology%22%5BJournal%5D)">Rezeptorpotential und nervenimpulse einzelner olfaktorischer sensillen der insektenantenne.</a> Journal of Comparative Physiology A: Neuroethology, Sensory, Neural, and Behavioral Physiology. 45, 405-412 (1962).</li>
<li>Blight, M. M., Pickett, J. A., Wadhams, L. J., Woodcock, C. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Antennal+perception+of+oilseed+rape+Brassica+napus+%28Brassicaceae%29+volatiles+by+the+cabbage+seed+weevil+Ceutorhynchus+assimilis+%28Coleoptera%2C+Curculionidae%29%5BTitle%5D)+AND+%22Journal+of+Chemical+Ecology%22%5BJournal%5D)">Antennal perception of oilseed rape Brassica napus (Brassicaceae) volatiles by the cabbage seed weevil Ceutorhynchus assimilis (Coleoptera, Curculionidae).</a> Journal of Chemical Ecology. 21, 1649-1664 (1995).</li>
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<li>Syed, Z., Leal, W. S. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Acute+olfactory+response+of+Culex+mosquitoes+to+a+human-+and+bird-derived+attractant%5BTitle%5D)+AND+%22Proceedings+of+the+National+Academy+of+Sciences%22%5BJournal%5D)">Acute olfactory response of Culex mosquitoes to a human- and bird-derived attractant.</a> Proceedings of the National Academy of Sciences. 106, 18803-18808 (2009).</li>
</ol>

No conflicts of interest declared.

Insect olfactory-mediated behaviors drive many different processes, including reproduction, host-site selection, and the identification of appropriate food resources. The study of these processes requires the ability to identify the volatiles emitted from the source, as well as the ability to identify those compounds that are mediating the behaviors. Complicating matters is that odors are comprised of tens to hundreds of individual compounds that together create a unique scent that is perceived differently than th...

<table><tbody><tr><td>Porapak Type Q 80-100 mesh</td><td>Waters</td><td>WAT027060</td><td></td></tr><tr><td>Reynolds Oven Bags</td><td>Reynolds</td><td></td><td></td></tr><tr><td>GC</td><td>Agilent</td><td>7820A</td><td></td></tr><tr><td>GC column</td><td>J&amp;amp;W Scientific, Folsom, CA, USA</td><td>DB-5 (30 m, 0.25 mm, 0.25 &amp;#956;m)</td><td></td></tr><tr><td>Analytical helium carrier gas</td><td>Praxair</td><td>HE K</td><td>1 cc/min</td></tr><tr><td>16-channel silicon electrode</td><td>Neuronexus Technologies</td><td>a4x4-3mm50-177</td><td></td></tr><tr><td>Fine wire NiCr, 0.012 mm diameter) </td><td>Sandvik Kanthal HP Reid</td><td>PX000004</td><td>For making custom tetrodes and stereotrodes</td></tr><tr><td>Pre-amplifier</td><td>Tucker-Davis System</td><td>PZ-2</td><td></td></tr><tr><td>Amplifier </td><td>Tucker-Davis System</td><td>RZ-2</td><td></td></tr><tr><td>Data acquisition system - OpenEx suite</td><td>Tucker-Davis System</td><td></td><td></td></tr><tr><td>Online spike-sorting software - SpikePac</td><td>Tucker-Davis System</td><td></td><td></td></tr><tr><td>Offline spike-sorting software - Mclust Spike-sorting toolbox </td><td>David Redish, Department of Neuroscience, University of Minnesota</td><td>Free download at &lt;a href=&quot;http://redishlab.neuroscience.umn.edu/MClust/MClust.html&quot; target=&quot;_blank&quot;&gt;http://redishlab.neuroscience.umn.edu/MClust/MClust.html&lt;/a&gt;</td><td>MATLAB toolbox</td></tr></tbody></table>

identification of olfactory volatiles using gas chromatography-multi-unit recordings (gcmr) in the insect antennal lobe

Identification of Olfactory Volatiles using Gas Chromatography-Multi-unit Recordings (GCMR) in the Insect Antennal Lobe

All organisms inhabit a world full of sensory stimuli that determine their behavioral and physiological response to their environment. Olfaction is especially important in insects, which use their olfactory systems to respond to, and discriminate amongst, complex odor stimuli. These odors elicit behaviors that mediate processes such as reproduction and habitat selection1-3. Additionally, chemical sensing by insects mediates behaviors that are highly significant for agriculture and human health, including pollination4-6, herbivory of food crops7, and transmission of disease8,9. Identification of olfactory signals and their role in insect behavior is thus important for understanding both ecological processes and human food resources and well-being.
	To date, the identification of volatiles that drive insect behavior has been difficult and often tedious. Current techniques include gas chromatography-coupled electroantennogram recording (GC-EAG), and gas chromatography-coupled single sensillum recordings (GC-SSR)10-12. These techniques proved to be vital in the identification of bioactive compounds. We have developed a method that uses gas chromatography coupled to multi-channel electrophysiological recordings (termed 'GCMR') from neurons in the antennal lobe (AL; the insect's primary olfactory center)13,14. This state-of-the-art technique allows us to probe how odor information is represented in the insect brain. Moreover, because neural responses to odors at this level of olfactory processing are highly sensitive owing to the degree of convergence of the antenna's receptor neurons into AL neurons, AL recordings will allow the detection of active constituents of natural odors efficiently and with high sensitivity. Here we describe GCMR and give an example of its use.
	Several general steps are involved in the detection of bioactive volatiles and insect response. Volatiles first need to be collected from sources of interest (in this example we use flowers from the genus Mimulus (Phyrmaceae)) and characterized as needed using standard GC-MS techniques14-16. Insects are prepared for study using minimal dissection, after which a recording electrode is inserted into the antennal lobe and multi-channel neural recording begins. Post-processing of the neural data then reveals which particular odorants cause significant neural responses by the insect nervous system.
	Although the example we present here is specific to pollination studies, GCMR can be expanded to a wide range of study organisms and volatile sources. For instance, this method can be used in the identification of odorants attracting or repelling vector insects and crop pests. Moreover, GCMR can also be used to identify attractants for beneficial insects, such as pollinators. The technique may be expanded to non-insect subjects as well.

In the GCMR assay using the M. lewisii floral scent, we inject 3 μl of the extract into the GC. The total number of volatiles eluting through the GC is typically 60-70 volatiles. The scent of M. lewisii is predominantly composed of monoterpenoids, including β-myrcene (acyclic) and α-pinene, with the remainder of the scent composed of six-carbon volatiles, such as 2-hexanol, and sesquiterpenoids that comprise &lt; 1% of the headspace.
 GCMR takes advan...

Olfactory cues mediate many different behaviors in insects, and are often complex mixtures comprised of tens to hundreds of volatile compounds. Using gas chromatography with multi-channel recording in the insect antennal lobe, we describe a method for the identification of bioactive compounds.

All  organisms inhabit a world full of sensory stimuli that determine their  behavioral and physiological response to their environment. Olfaction is ...

The overall goal of this procedure is to identify biologically effective odorants in complex sense through recordings in the bumblebee brain. This is accomplished by first collecting behaviorally effect sense, and second, preparing the gas chromatograph and multichannel recording systems for the experiment. The third step is to prepare and dissect the bumblebee brain for the neural recordings in the antenna of factory lobe.The experiment is then conducted by inserting the electrodes into the an antenna lobe and measuring responses to puffed volatiles by analysis of the neural activity in response to complex sense and their individual constituents. Biologically active odorants obtained by gas chromatography can be identified. So the main advantage of this technique relative to other techniques like G-C-E-A-G, is the sensitivity of antenna load neurons and the ability to characterize how neurons in the brain respond to specific floral volatiles.Visual demonstration of this method is critical as a combined electrophysiological and chemical analytical steps are difficult to learn because of the electrophysiological preparation recording technique and the necessary steps for collecting

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JoVE Journal

Neuroscience

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).

Single Sensillum Recordings in the Insects Drosophila melanogaster and Anopheles gambiae

Multielectrode array (MEA) recordings provide a method for studying the electrical activity of large populations of neurons.  Here, we present the details of a MEA preparation to record from the mouse vomeronasal epithelium while simultaneously stimulating the tissue.

Multielectrode Array Recordings of the Vomeronasal Epithelium

Insect olfactory systems provide unique opportunities for recording odorant-induced responses in the forms of electroantennograms (EAG) and single sensillum recordings (SSR), which are summed responses from all odorant receptor neurons (ORNs) located on the antenna and from those housed in individual sensilla, respectively.

Electrophysiological Measurements from a Moth Olfactory System

A method to rapidly screen host plant volatiles by measurement of the electrophysiological response of adult navel orangeworm (Amyelois transitella) antennae to single components and blends via electroantennographic analysis is demonstrated.

Electroantennographic Bioassay as a Screening Tool for Host Plant Volatiles

We demonstrate variations of the extracellular multi-unit recording technique to characterize odor-evoked responses in the first three stages of the invertebrate olfactory pathway. These techniques can easily be adapted to examine ensemble activity in other neural systems as well.

Multi-unit Recording Methods to Characterize Neural Activity in the Locust (Schistocerca Americana) Olfactory Circuits

We describe a protocol for using insect antennae in the form of electroantennograms (EAGs) on autonomous robots. Our experimental design allows stable recordings within a day and resolves individual odor patches up to 10 Hz. The efficiency of EAG sensors for olfactory searches is demonstrated in driving a robot toward an odor source.

Using Insect Electroantennogram Sensors on Autonomous Robots for Olfactory Searches

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.

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

Minor workers of the ant species Colobopsis explodens are dissected to isolate the wax-like content stored in their hypertrophied mandibular gland reservoirs for subsequent solvent-extraction and analysis by gas chromatography-mass spectrometry. The annotation and identification of volatile constituents using the open-source software MetaboliteDetector is also described.

Isolation of Mandibular Gland Reservoir Contents from Bornean 'Exploding Ants' (Formicidae) for Volatilome Analysis by GC-MS and MetaboliteDetector

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

Single Sensillum Recordings for Locust Palp Sensilla Basiconica

Here, we present a protocol for collecting the floral fragrance volatiles from blooming flowers, using a non-destructive sampling procedure.

Rapid Collection of Floral Fragrance Volatiles using a Headspace Volatile Collection Technique for GC-MS Thermal Desorption Sampling

Physiologically, odorant receptors are activated by odorant molecules inhaled in the vapor phase. However, most in vitro systems utilize liquid phase odorant stimulation. Here, we present a method that allows real-time in vitro monitoring of odorant receptor activation upon odorant stimulation in vapor phase.

Real-time In Vitro Monitoring of Odorant Receptor Activation by an Odorant in the Vapor Phase

Learn to identify biologically active odorants in complex scents using gas chromatography and multi-unit recordings in the bumblebee antennal lobe. This method enables precise neural characterization of floral volatiles.

Identification of Olfactory Volatiles using Gas Chromatography-Multi-unit Recordings (GCMR) in the Insect Antennal Lobe

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