We thank U. Heberlein and A. Devineni for long-lasting discussions and technical advice. We also thank the Shohat-Ophir lab members, A. Benzur, L. Kazaz, and O. Shalom, for the help with demonstrating the method. Special appreciation goes to Eliezer Costi for establishing the fly systems in the lab. This work was supported by the Israel Science Foundation (384/14) and the Marie Curie Career Integration Grants (CIG 631127).

Note: General overview of the experimental design: The experimental design includes an adapted protocol for courtship suppression7-9 in which male flies are exposed to rewarding and nonrewarding experiences in 3 consecutive training sessions over the course of 4 d. At the end of the experience phase, the flies are tested in a two-choice voluntary ethanol consumption assay for 3&#160;- 4 d. The protocol herein includes several preparatory steps, some of which can be done in advance to be used in more than one experiment, while others should take place in a timely manner before the beginning of the experiment (Table 1).
1. Preparatory Steps
<ol>
	<li>Preparing the capillary feeder system
	<ol>
		<li>Heat a 27&#160;G needle and use it to puncture small holes along a vial (Figure 1).</li>
		<li>Cut the vial plug in half (crosswise) using a razor blade. Mark four points on the surface of the plug, creating a square shape to position the capillary holders into. Use an 18&#160;G needle to make 4 holes through the plug (Figure 1b).</li>
		<li>Use a razor blade to cut micropipets so that they can firmly hold 5 &#181;L glass capillaries, which serve as adaptors.</li>
		<li>Insert 4 capillary adaptors into the prepared plugs.</li>
		<li>Mark the position of the 2 ethanol- and&#160;two nonethanol-containing capillaries on the plug. 
		Note: It is recommended to keep the positions of the 2 types of capillaries consistent across all vials. Pay attention to the size of the holes, as large holes allow the escape of flies out of the vials. In addition, it is recommended to use the smoother side of the plug (usually opposite the cut side) as the side that faces down when inserted into the vial, as cutting the plug creates some small, loose fibers that the flies can get tangled in.</li>
		<li>Prepare a large number of vials and adaptors to be used for the capillary feeder system (CAFE) experiments described in step 2.3.</li>
	</ol>
	</li>
	<li>Preparing small glass food vials
	<ol>
		<li>A day before collecting the flies (step 1.4), arrange 200 glass vials on microcentrifuge tube racks. Melt fly food (according to the cornmeal molasses recipe, see the Table of Materials) using a microwave. Pour 2 mL of fly food into the glass vials (try not to smear the food on the vial walls). Let the food harden, and cover the vials with plastic wrap. 
		NOTE: The glass vials containing the food can be kept at 4 &#176;C for several weeks.</li>
		<li>On the day of fly collection, take the vials out of the refrigerator and let them reach RT before using them to house flies. 
		NOTE: If food vials are several weeks old, make sure that the food is still intact and not detached from the vial, as flies can be trapped in the cracks between the food and the glass.</li>
	</ol>
	</li>
	<li>Making stock food solution for the capillary feeder assay
	<ol>
		<li>To prepare the stock food solution (5% sucrose and 5% yeast extract), dissolve 5.88 g of yeast extract and 5.88 g of sucrose in 100 mL of distilled water. 
		NOTE: The stock solution is highly prone to contamination. Therefore, it is recommended to autoclave it (121 &#176;C, 30 min, and without a drying cycle) and aliquot it into 850&#160;&#181;L working aliquots to be kept at 4 &#176;C until further use. The concentration of the ingredients in the stock solution is 5.88% and will reach the final concentration of 5% after the addition of 15% ethanol or water (150 &#181;L into 850 &#181;L of premade food solution) just before its use in step 2.3.</li>
	</ol>
	</li>
	<li>Collecting experimental flies
	<ol>
		<li>Collect 200 na&#239;ve male flies using a CO2 pad. 
		Note: Use any lab strain relevant for the experimental question. 250 flies can be easily collected from five bottles of flies at their eclosion pick phase. When collecting the flies, pay careful attention to collect flies that have recently eclosed (virgin-looking flies: bright flies with a meconium spot on their abdomen). Experimental flies should be kept singly in small glass vials containing food and aged to 3 - 4 d&#160;old before being used in the experiment.</li>
		<li>Use soft plugs to close the vials. 
		NOTE: The same soft plugs will be very useful for the training phase when using mouth aspiration to insert females into and out of the vials during the experience phase.</li>
	</ol>
	</li>
	<li>Collecting trainer flies 
	NOTE: All collected flies should be kept in a 12&#160;h/12&#160;h light/dark incubator at 25 &#176;C and 70% Relative Humidity (RH). The 12&#160;h/12&#160;h light/dark cycle can be changed to a convenient starting time.
	<ol>
		<li>Virgin female trainer flies
		<ol>
			<li>Collect 500 virgin female trainer flies from a WT stock or a virginator stock for use as virgin receptive females. Keep the female flies in groups of 25 per regular-size food vial, and allow them to age to 3 - 4 d old before using them in the experiment.</li>
		</ol>
		</li>
		<li>Mated female trainer flies
		<ol>
			<li>Collect 300 virgin female flies from a WT stock or a virginator stock to undergo mating before the training phase (step 1.6.1). 
			NOTE: Female flies are kept in groups of 10 females per regular-size food vial and aged to 3 - 4 d old before being used in the experiment.</li>
		</ol>
		</li>
		<li>Male flies used to generate mated female trainer flies
		<ol>
			<li>Collect 150 male flies (not necessarily virgin). 
			NOTE: Flies are kept in groups of 15 males per regular-size food vial and aged to 3 - 4 d old before being paired with virgin female flies to create the mated trainer females.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Generating mated female trainer flies
	<ol>
		<li>To generate mated female flies to be used as trainers, pair groups of 10 virgin female flies with 15 male flies by flipping one male-containing vial into a female-containing vial 16 - 18 h before the training phase (step 2.1)10. 
		NOTE: This should normally take place the evening before the training session. The 1.5:1 ratio between male flies to female flies assures that all females will be mated.</li>
		<li>On the day of the experiment, separate the mated females from the males by aspirating the males out of the vial using a mouth aspirator. Perform this right before the beginning of each training day.</li>
	</ol>
	</li>
</ol>
2. Experimental Steps
<ol>
	<li>Setting up the experience phase
	<ol>
		<li>Start the experiment as close as possible to the beginning of the light phase in the incubator. Place the trainer females (both virgin and mated) in the behavior chamber. 
		NOTE: It is recommended to perform the experiment in a behavior chamber, or any secluded environment that is quiet and set to 25 &#176;C and 60 - 65% RH. Keeping humidity over 50% is very important, since courtship and mating behaviors depend on pheromone sensing, which is known to be sensitive to humidity.</li>
	</ol>
	</li>
	<li>Exposing male flies to rewarding and nonrewarding experiences
	<ol>
		<li>Arrange the glass vials containing the single male flies on microcentrifuge racks, positioning the vials along the margins of the rack. 
		NOTE: This arrangement allows the experimenter to easily observe the pairs of flies that undergo copulation without taking the vials out of the rack.</li>
		<li>Prepare (as described in step 2.2.1) 2 groups of 100 glass vials containing single male flies on separate racks for males undergoing rewarding and nonrewarding mating experiences (i.e.&#160;rejected and mated).</li>
		<li>Aspirate trainer females and add them to each vial containing the male flies. Set the timer for 1 h. Starting with the rejected group, add a mated female to each vial. Then, move on to the males to be mated and add a virgin female to each vial.</li>
		<li>Watch the mating encounters closely to make sure that the males interacting with virgin females mate successfully within the first hour and that the males interacting with the previously-mated females do not mate. To monitor the rejected cohort over the course of 1 h, set a second timer for 15 min and watch the males every 15 min.</li>
		<li>Discharge the males from the rejected cohort that managed to mate and males from the mated cohort that did not end up mating by the end of the first training session.</li>
		<li>Finish the first training session by aspirating out the previously-mated female trainers into a regular fly food vial, and keep them for the next conditioning session. Follow this step by gently aspirating the females from the mated male group.</li>
		<li>Let the flies rest for 1 h.</li>
		<li>Repeat steps 2.2.3 - 2.2.7 twice.</li>
		<li>Repeat the training session in steps 2.2.3 - 2.2.8 each day for 3 more d.</li>
	</ol>
	</li>
	<li>Recording consumption (CAFE)
	<ol>
		<li>At the end of the last conditioning session (fourth day), aspirate the single males and group them into the capillary feeder vials. Use a soft plug to cover the capillary feeder vial while inserting the flies, and replace it quickly with the ready-made capillary feeder plug after all the flies have been inserted. Group 6 - 8 flies from each of the experimental groups into a vial, creating no less than 8 vials per condition.</li>
		<li>Wet the plugs by gently adding 5 mL of water to the top of the plug. Be careful while adding the water to avoid spillage into the vials. Add equal amount of water to each vial. 
		NOTE: This step is done to reduce evaporation from the capillaries. Therefore, it is repeated every day for the rest of the experiment. Depending on the relative humidity, the following days may require less water to be added to the plugs.</li>
		<li>Prepare two separate food solutions by adding ethanol or water to the stock food aliquots to create a final concentration of 15%.</li>
		<li>To fill the capillaries with the two food solutions, create 5&#160;&#181;L liquid food drops on a laboratory film strip and allow the solution to fill the capillary until it reaches the 5&#160;&#181;L mark. Make sure to use the clear end of the capillary, which is close to the 5&#160;&#181;L black mark line. 
		NOTE: To fill several capillaries at once, it is possible to connect 6 - 8 capillary adaptors together and use them as an insert to hold the capillaries.</li>
		<li>Tap the capillaries gently on the paraffin strip to position the food solution exactly at the black mark. Seal the capillaries by dipping the end of each capillary into small drops of mineral oil. This step minimizes potential evaporation of the food solution.</li>
		<li>Insert two ethanol-containing capillaries and two nonethanol containing capillaries through the 4 adaptors/holders in the plug until the exposed sides of the capillaries barely peek from the interior of the vial (1 mm or less from the plug surface). 
		NOTE: Keeping the opening of the capillaries close to the wet plug reduces evaporation and allows easy access to the food, as flies normally sit on the plugs and climb down on the exposed capillary to feed.</li>
		<li>In addition to vials that contain experimental flies, prepare a mock vial without flies. This control serves to assess natural evaporation. 
		NOTE: Try to maintain relatively equal positioning of the capillary opening compared to the plugs, as differences can lead to variable evaporation and to misleading consumption data. Maintain adequate humidity during the experiment and position the capillary openings as closely as possible to the wet plug, as low humidity and large distance from the wet plug can both result in uncontrolled evaporation.</li>
		<li>Record the relative position of the liquid in each of the capillaries with respect to the black mark line in mm using a ruler, and write these values down. 
		NOTE: If the solution is positioned exactly at the black line, the value should equal zero, and if it is above or below, it should be positive or negative values, respectively. The initial levels of the liquid set the reference points for the final O/N consumption values.</li>
		<li>Set the vials back in the incubator for 24 h. Replace the capillaries at a constant time throughout the entire experiment.</li>
		<li>Remove the capillaries gently from the vials and measure the levels of liquid with respect to the black marking line.</li>
		<li>Carefully check the liquid level in the mock vial. 
		NOTE: If the levels dropped more than 2 mm, it indicates that evaporation is high and the consumption levels are not reliable.</li>
		<li>Dampen the plugs gently with 2 mL of water and insert a new set of capillaries, as indicated in steps 2.3.3 - 2.3.10. Set the vials back in the incubator for 24 h.</li>
	</ol>
	</li>
	<li>Determining preference
	<ol>
		<li>Calculate the total consumption of each capillary by subtracting the final level from the initial level at the starting point.</li>
		<li>Combine the values of both capillaries with the same food (i.e.&#160;nonethanol capillaries separately from ethanol-containing capillaries).</li>
		<li>Calculate ethanol preference by subtracting the amount consumed from the non-ethanol capillaries from the amount consumed from the ethanol-containing capillaries and divide the value by the total consumption values from all the capillaries of the same vial.</li>
		<li>Average the preference indexes of all vials of the same experimental group. 
		<img alt="Equation1" src="/files/ftp_upload/54910/54910equation1.jpg" /> 
		NOTE: Nonethanol 1 (NE1), Nonethanol 2 (NE2), Ethanol 1 (E1), Ethanol 2 (E2), Total nonethanol (Total NE) = NE1 + NE2, Total ethanol (Total E) = E1 + E2, Total sum consumption (Total Sum) = Total NE + Total E, and Ethanol preference Index (PI)</li>
	</ol>
	</li>
</ol>

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The authors have nothing to disclose.

Here, we illustrate the details of an integrated approach to measure alterations in reward-seeking behavior, based on previous work described by Devineni et al.6 and Shohat-Ophir et al5. The first section of the protocol uses different types of sexual interactions as the experience input, and the second section uses a two-choice feeding assay to assess the effect of experience on the preference to consume ethanol.
As shown by Devineni et al.6, ethanol self-administration in flies is a robust behavior, characterized at first by low and variable preference that increases and becomes more consistent over time. The developing preference may reflect a process through which flies learn to associate the pharmacological effect of ethanol with its position, in spite of its unpleasant taste6 and the aversive responses known to occur during initial exposure to ethanol vapors11. Changing the position of the ethanol-containing capillary on a daily basis results in a constant level of preference, strongly demonstrating the role of learning and suggesting that the flies leave chemical cues next to the preferred capillaries12. In addition, the shape, the slope, and the starting point of the preference curve can be slightly different between experiments, but the overall magnitude of difference between the groups of flies that are exposed to rewarding and non-rewarding experiences is preserved across experiments.
The question of whether flies display preference to consume ethanol for its caloric value or pharmacological properties is still under debate and was examined in the last few years by several independent studies (for a review, see Devineni et al.)13. Taking into account the results obtained from these studies, it is likely that the caloric value of ethanol contributes to the pharmacological effect of ethanol and is not the main reason for the development of preference to consume ethanol.
As this protocol reflects voluntary consumption in groups of flies, the technique is limited to cumulative changes in consumption over at least several hours and is not sensitive enough to reflect short temporal changes in consumption over short time frames (minutes). Other feeding assays, such as FLIC14, flyPAD15, and EXPRESSO16, that can measure the frequency of feeding events and their bout length are technologically superior to the CAFE assay and can therefore provide high-content temporal data of feeding and ethanol preference. Still, compared to other simple two-choice assays that are based on measuring the ingestion of food mixed together with food dyes, the CAFE approach allows the accurate and uninterrupted monitoring of consumption data over several days17,18.
Although described together, each section can be used separately in future applications. The training phase can be used for further downstream analyses of plasticity-related events using real-time PCR, RNAseq, proteomic, and metabolomic screens. Following the training phase, it is also possible to use FLIC14, flyPAD15, or EXPRESSO16 to achieve higher resolution in the consumption data. The two-choice ethanol consumption assay can also serve to study the effect of other external stimuli, such as stress, on the internal state19,20. Additionally, using neurogenetic tools that control neuronal activity as an input experience and ethanol consumption as an output behavior, it can be used to dissect the neuronal circuits that encode internal reward.
Even though the described protocol is relatively simple and does not require sophisticated equipment, there are critical steps that require the most attention to ensure reproducible results. First, it is important to start the experiment with large male flies that eclosed from healthy fly bottles. Secondly, it is essential to make sure that the mated cohort indeed undergo mating and that the rejected cohort do not manage to mate. Lastly, it is important to maintain a well-humidified environment for the entire experiment, with an emphasis on the consumption part. This includes watering the plugs every day with equal amounts of water and keeping the capillary ends in close proximity to the wet plugs.

Modification of behavior in response to experience allows animals to adjust their behavior to changes in their environment1. During this process, animals integrate their internal physiological state with the changing conditions of the external environment and subsequently choose one action over another to increase their chances of survival and reproduction. Reward systems evolved to motivate behaviors that are required for the survival of individuals and species by reinforcing behaviors that enhance immediate survival, such as eating or drinking, or those that ensure long-term survival, such as sexual behavior or caring for offspring2. Artificial compounds such as drugs of abuse also affect reward systems by co-opting neural pathways that mediate natural rewards2.
During the last two decades, the fruit fly Drosophila melanogaster has been established as a promising model for studying the molecular and neuronal mechanisms that are shaping the effects of ethanol on behavior3,4.
Previously, we have identified a subset of peptidergic neurons in flies (NPF/NPF receptor (R) neurons) that couple natural rewards, such as sexual experience, to the motivation of obtaining drug rewards5. NPF expression is sensitive to both sexual experiences and to drug rewards, such as ethanol intoxication. Changes in NPF expression levels are converted to alterations in ethanol self-administration5, where high NPF reduces and low NPF increases the preference to consume ethanol. Activating NPF neurons is rewarding for flies, as they display strong preference for an odor paired with the activation, which is also reflected by reduced ethanol consumption. More importantly, activation of NPF neurons interferes with the ability of flies to form a positive association between ethanol intoxication and an odor cue. The causal link between the NPF/R system, reward memory, and ethanol consumption suggests that one can use ethanol self-administration as a measure for changes in reward states5.
In this publication we demonstrate an integrated approach for tapping into the fly natural reward system and assaying changes in reward states. The approach consists of two separate parts, a training protocol for manipulating natural reward-related experiences, followed by a two-choice capillary feeder assay (CAFE) to assess ethanol self-administration as an estimate for changes in reward states. The CAFE assay is analogous to the two-bottle choice assays used in rodent studies for drug self-administration and has been shown to reflect certain properties of addiction-like behavior in flies6.

<table><tbody><tr><td>Polystyrene 25 x 95 mm Vials</td><td>FlyStuff</td><td>32-109</td><td></td></tr><tr><td>narrow plastic vials flugs</td><td>FlyStuff</td><td>42-102</td><td></td></tr><tr><td>Disposable Sterile Needle 18 G and 27 G&amp;nbsp;</td><td>can be acquired by any company</td><td></td><td>1.20 X 38 mm (18 G x 1 1/2&quot;) , 0.40 X 13 mm (27 G x 1/2&quot;)</td></tr><tr><td>10 x 75 mm Borosilicate Glass Disposable Culture Tubes</td><td>kimble chase</td><td>73500-1075</td><td></td></tr><tr><td>calibrated pipets 5 &amp;#956;L</td><td>VWR</td><td>53432-706</td><td>color coded white to contain 5 &amp;#956;L</td></tr><tr><td>Mineral Oil&amp;nbsp;</td><td>Sigma-Aldrich&amp;nbsp;</td><td>M5904</td><td></td></tr><tr><td>Sucrose, Molecular Biology Grade</td><td>CALBIOCHEM</td><td>573113</td><td></td></tr><tr><td>Yeast extract Powder for microbiology</td><td>can be acquired by any company</td><td></td><td></td></tr><tr><td>Ethanol</td><td>Sigma-Aldrich&amp;nbsp;</td><td>32221</td><td></td></tr><tr><td>standard pipette Tips (micro-pipetts)</td><td>ThermScientific</td><td>T114R-Q</td><td>volume: 0.1 - 20 &amp;#956;L (ultramicro)</td></tr><tr><td>IDENTI-PLUGS (Foam Tube Plugs)</td><td>Jaece</td><td>L800-A</td><td>fits opening 6 - 13 mm</td></tr><tr><td>IDENTI-PLUGS (Foam Tube Plugs)</td><td>Jaece</td><td>L800-D</td><td>fits opening 35 - 45 mm</td></tr><tr><td>virginator fly stock&amp;nbsp;</td><td>bloomington drosophila stock center</td><td>#24638</td><td></td></tr><tr><td>Narrow Vials, Tray Pack (PS)</td><td>Genesee Scientific Corporation</td><td>&amp;nbsp;# 32-109BR</td><td></td></tr><tr><td>Drosophila Media Recipes and Methods</td><td>Bloomington Drosophila Stock Center</td><td>http://flystocks.bio.indiana.edu/Fly_Work/media-recipes/molassesfood.htm</td><td></td></tr><tr><td>propionic acid</td><td>Sigma-Aldrich&amp;nbsp;</td><td>P5561</td><td></td></tr><tr><td>phosphoric acid</td><td>Sigma-Aldrich&amp;nbsp;</td><td>W290017</td><td></td></tr><tr><td>Methl 4-Hydroxybenzoate</td><td>Sigma-Aldrich&amp;nbsp;</td><td>H3647</td><td></td></tr><tr><td>Agar Agar</td><td>can be acquired by any company</td><td></td><td></td></tr><tr><td>corn meal</td><td>can be acquired by any company</td><td></td><td></td></tr><tr><td>Grandma&#039;s molasses</td><td>B&amp;amp;G Foods, Inc</td><td>not indicated</td><td></td></tr><tr><td>instant dry yeast</td><td>can be acquired by any company</td><td></td><td></td></tr></tbody></table>

a simple way to measure alterations in reward-seeking behavior using drosophila melanogaster

We describe a protocol for measuring ethanol self-administration in fruit flies (Drosophila melanogaster) as a proxy for changes in reward states. We demonstrate a simple way to tap into the fly reward system, modify experiences related to natural reward, and use voluntary ethanol consumption as a measure for changes in reward states. The approach serves as a relevant tool to study the neurons and genes that play a role in experience-mediated changes of internal state. The protocol is composed of two discrete parts: exposing the flies to rewarding and nonrewarding experiences, and assaying voluntary ethanol consumption as a measure of the motivation to obtain a drug reward. The two parts can be used independently to induce the modulation of experience as an initial step for further downstream assays or as an independent two-choice feeding assay, respectively. The protocol does not require a complicated setup and can therefore be applied in any laboratory with basic fly culture tools.

FPreviously, Devineni et al. showed that when fruit flies are given the choice to consume ethanol-containing food, they display a strong preference for ethanol-containing food over nonethanol containing food6. Shown here are some representative results we obtained when assaying the innate ethanol preference of na&#239;ve male flies that did not undergo the training protocol.
Na&#239;ve Canton S male flies were collected upon eclosion, aged until 4-day-old, and assayed for their innate preference to consume ethanol over the course of 4 d (Figure 2). Analyzing the amounts consumed from ethanol- and nonethanol-containing solutions shows that flies exhibit a robust preference for consuming 15% ethanol food over nonethanol food (Figure 2).
Using opposing sexual experiences, we have previously demonstrated that male flies that were allowed to mate in groups (&#34;mated-grouped&#34;) display lower ethanol preference than singly-housed males that were rejected by previously-mated females (&#34;rejected-isolated&#34;). We used several controls to uncouple the housing experience from the mating-related experience and showed that the differential preference results from the mating experience5.
Using the training protocol described here, we generated singly-mated and rejected male flies that underwent similar housing and mating regimes. Single male Canton S flies were subjected over the course of 4 d&#160;to disparate mating experiences. One cohort of males was allowed to interact and mate with virgin female flies (single mated cohort), and the other cohort was trained with previously-mated female flies (single rejected cohort). Following the training phase, the single males from the two cohorts were grouped (8/vial) and placed in the capillary feeder vials; their voluntary ethanol consumption was recorded for 4 d&#160;(Figure 3A). The preference to consume ethanol was calculated from the consumption data using the formula in step 2.4 (Figure 3B). Positive values indicate preference for ethanol-containing food, and negative values indicate aversion to ethanol-containing food.
The present experiment supports our previous findings, suggesting that sexual experience, and not housing condition, modulates ethanol consumption. Successful mating increases internal reward levels, which in turn lowers ethanol consumption. Rejections, perceived as a lack of reward, lead to an increase in reward-seeking behavior (Figure 3B).
<img alt="Figure 1" src="/files/ftp_upload/54910/54910fig1.jpg" /> 
Figure 1. Schematic of the Capillary Feeder System (CAFE). (a) Schematics of the perforated vial with holes to equilibrate pressure and humidity. (b) Schematics of the cut-in-half plug that serves as the base for the insertion of the capillaries. (c) Schematics of shape and location of the adaptors serving to hold the capillaries. <a href="http://cloudflare.jove.com/files/ftp_upload/54910/54910fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" src="/files/ftp_upload/54910/54910fig2.jpg" /> 
Figure 2. An Example of innate Preference to Consume Ethanol. Na&#239;ve WT males were grouped in groups of 8 males/vial, and their consumption of ethanol- and nonethanol-containing solutions were recorded over the course of 96 h. The flies consumed a larger amount of 15%&#160;ethanol containing food (**P &#60;0.01, ***P &#60;0.001, two-way repeated measures ANOVA with Bonferroni post-tests, n = 8). Data shown are the mean + SEM or mean - SEM. <a href="http://cloudflare.jove.com/files/ftp_upload/54910/54910fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" src="/files/ftp_upload/54910/54910fig3.jpg" /> 
Figure 3. Opposing Mating Experiences mModulate Ethanol Preference. (A) Schematic of the combined protocol. Single virgin WT males are allowed to mate with virgin females or are subjected to 3x 1h courtship-suppression training sessions (depicted as &#34;T&#34;) spaced by 1 h of rest (depicted as &#34;R&#34;). Training is repeated for 4 d. At the end of each day, the flies are placed in the incubator (depicted as &#34;O.N&#34;). After 4 d of training, the males were placed in vials where they could choose to feed from capillaries containing food solutions with or without 15% ethanol. (B) Single rejected males exhibited higher ethanol preference than single mated males (**P &#60;0.01, two-way repeated-measures ANOVA with Bonferroni post-tests, n = 9, comparisons are between treatment groups across 3 d&#160;after the end of training). Data shown are the mean + SEM or mean - SEM. <a href="http://cloudflare.jove.com/files/ftp_upload/54910/54910fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table fo:keep-together.within-page="1">
	<tbody>
		<tr>
			<td>Reference section&#160;</td>
			<td>&#160;&#160; Notes</td>
		</tr>
		<tr>
			<td>1.1</td>
			<td>Can be used in many experiments</td>
		</tr>
		<tr>
			<td>1.2</td>
			<td>Can be kept in 4 &#176;C for several weeks</td>
		</tr>
		<tr>
			<td>1.3</td>
			<td>Keep in 4 &#176;C after autoclave</td>
		</tr>
		<tr>
			<td>1.4</td>
			<td>Aged to 3 - 4 d before being used in the experiment</td>
		</tr>
		<tr>
			<td>1.5</td>
			<td>This step should take place the evening before each training session</td>
		</tr>
		<tr>
			<td>2.1</td>
			<td>This step should take place the morning of each training session&#160;</td>
		</tr>
		<tr>
			<td>2.2</td>
			<td>To be repeated in 3 consecutive training sessions over the course of 4 d</td>
		</tr>
		<tr>
			<td>2.3</td>
			<td>Dump the plugs with water, measure consumption and replace capillaries over the course of 4 d</td>
		</tr>
		<tr>
			<td>2.4</td>
			<td>This step is done each time before replacing the capillaries during the two-choice assay</td>
		</tr>
	</tbody>
</table>
Table 1. An overview of the protocol depicting the order and time flow for the different steps.

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A Simple Way to Measure Alterations in Reward-seeking Behavior Using Drosophila melanogaster

We describe a protocol for inducing rewarding and nonrewarding experiences in fruit flies (Drosophila melanogaster) using voluntary ethanol consumption as a measure for changes in reward states.

A Simple Way to Measure Alterations in Reward-seeking Behavior Using Drosophila melanogaster

We describe a protocol for measuring ethanol self-administration in fruit flies (Drosophila melanogaster) as a proxy for changes in reward states. We ...

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Nanyang Technological University

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8.3K Views.  Bar-Ilan University. We describe a protocol for inducing rewarding and nonrewarding experiences in fruit flies (Drosophila melanogaster) using voluntary ethanol consumption as a measure for changes in reward states.

Video: A Simple Way to Measure Alterations in Reward-seeking Behavior Using Drosophila melanogaster

Combining Quantitative Food-intake Assays and Forcibly Activating Neurons to Study Appetite in Drosophila

Food consumption is under the tight control of the brain, which integrates the physiological status, palatability, and nutritional contents of the food, and issues commands to start or stop feeding. Deciphering the processes underlying the decision-making of timely and moderate feeding carries major implications in our understanding of physiological and psychological disorders related to feeding control. Simple, quantitative, and robust methods are required to measure the food ingestion of animals after experimental manipulation, such as forcibly increasing the activities of certain target neurons. Here, we introduced dye-labeling-based feeding assays to facilitate the neurogenetic study of feeding control in adult fruit flies. We review available feeding assays, and then describe our methods step-by-step from setup to analysis, which combine thermogenetic and optogenetic manipulation of neurons controlling feeding motivation with dye-labeled food intake assay. We also discuss the advantages and limitations of our methods, compared with other feeding assays, to help readers choose an appropriate assay.

Combining Quantitative Food-intake Assays and Forcibly Activating Neurons to Study Appetite in Drosophila

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Behavior

Appetitive Associative Olfactory Learning in Drosophila Larvae

In the following we describe the methodological details of appetitive associative olfactory learning in Drosophila larvae. The setup, in combination with genetic interference, provides a handle to analyze the neuronal and molecular fundamentals of specifically associative learning in a simple larval brain.
Organisms can use past experience to adjust present behavior. Such acquisition of behavioral potential can be defined as learning, and the physical bases of these potentials as memory traces1-4. Neuroscientists try to understand how these processes are organized in terms of molecular and neuronal changes in the brain by using a variety of methods in model organisms ranging from insects to vertebrates5,6. For such endeavors it is helpful to use model systems that are simple and experimentally accessible. The Drosophila larva has turned out to satisfy these demands based on the availability of robust behavioral assays, the existence of a variety of transgenic techniques and the elementary organization of the nervous system comprising only about 10,000 neurons (albeit with some concessions: cognitive limitations, few behavioral options, and richness of experience questionable)7-10.
Drosophila larvae can form associations between odors and appetitive gustatory reinforcement like sugar11-14. In a standard assay, established in the lab of B. Gerber, animals receive a two-odor reciprocal training: A first group of larvae is exposed to an odor A together with a gustatory reinforcer (sugar reward) and is subsequently exposed to an odor B without reinforcement 9. Meanwhile a second group of larvae receives reciprocal training while experiencing odor A without reinforcement and subsequently being exposed to odor B with reinforcement (sugar reward). In the following both groups are tested for their preference between the two odors. Relatively higher preferences for the rewarded odor reflect associative learning - presented as a performance index (PI). The conclusion regarding the associative nature of the performance index is compelling, because apart from the contingency between odors and tastants, other parameters, such as odor and reward exposure, passage of time and handling do not differ between the two groups9.

Appetitive Associative Olfactory Learning in Drosophila Larvae

Drosophila larvae are able to associate odor stimuli with gustatory reward. Here we describe a simple behavioral paradigm that allows the analysis of appetitive associative olfactory learning.

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A Single-fly Assay for Foraging Behavior in Drosophila

For many animals, hunger promotes changes in the olfactory system in a manner that facilitates the search for appropriate food sources. In this video article, we describe an automated assay to measure the effect of hunger or satiety on olfactory dependent food search behavior in the adult fruit fly Drosophila melanogaster. In a light-tight box illuminated by red light that is invisible to fruit flies, a camera linked to custom data acquisition software monitors the position of six flies simultaneously. Each fly is confined to walk in individual arenas containing a food odor at the center. The testing arenas rest on a porous floor that functions to prevent odor accumulation. Latency to locate the odor source, a metric that reflects olfactory sensitivity under different physiological states, is determined by software analysis. Here, we discuss the critical mechanics of running this behavioral paradigm and cover specific issues regarding fly loading, odor contamination, assay temperature, data quality, and statistical analysis.

A Single-fly Assay for Foraging Behavior in Drosophila

In this video article, we describe an automated assay to measure the effect of hunger or satiety on olfactory dependent food search behavior in the adult fruit fly Drosophila melanogaster.

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Analysis of Sugar-Induced Foraging Behavior in Drosophila

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Foraging behavior is essential for the survival of organisms as it enables them to locate and acquire essential food resources. In Drosophila, hunger triggers a distinct search behavior following the consumption of small quantities of a sugar solution. This report presents a simple experimental setup to study sugar-elicited search behavior with the aim of uncovering the underlying mechanisms. Minute quantities of concentrated sugar solution elicit sustained searching behavior in flies. The involvement of path integration in this behavior has been established, as flies utilize their trajectory to return to the sugar location. The most recent findings provide evidence of temporal modulation in the initiation and intensity of the search behavior after sugar intake. We have also used this setup for artificial activation of specific taste-receptor neurons in the pharynx, which elicits the search behavior. The Drosophila neurogenetic toolkit offers a diverse array of tools and techniques that can be combined with the sugar-elicited search behavior paradigm to study the neural and genetic mechanisms underlying foraging. Understanding the neural basis of hunger-driven searching behavior in flies contributes to the field of neurobiology as a whole, offering insights into the regulatory mechanisms that govern feeding behaviors not only in other organisms but also in humans.

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This protocol describes a behavioral assay for recording sugar-elicited search behavior using Drosophila melanogaster. The assay can be utilized to study feeding and foraging-related behaviors, as well as the underlying neuronal mechanisms.

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In their natural environment, insects such as the vinegar fly Drosophila melanogaster are bombarded with a huge amount of chemically distinct odorants. To complicate matters even further, the odors detected by the insect nervous system usually are not single compounds but mixtures whose composition and concentration ratios vary. This leads to an almost infinite amount of different olfactory stimuli which have to be evaluated by the nervous system.
To understand which aspects of an odor stimulus determine its evaluation by the fly, it is therefore desirable to efficiently examine odor-guided behavior towards many odorants and odor mixtures. To directly correlate behavior to neuronal activity, behavior should be quantified in a comparable time frame and under identical stimulus conditions as in neurophysiological experiments. However, many currently used olfactory bioassays in Drosophila neuroethology are rather specialized either towards efficiency or towards resolution.
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High-resolution Quantification of Odor-guided Behavior in Drosophila melanogaster Using the Flywalk Paradigm

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High Throughput Assay to Examine Egg-Laying Preferences of Individual Drosophila melanogaster

Recently, egg-laying preference of Drosophila has emerged as a genetically tractable model to study the neural basis of simple decision-making processes. When selecting sites to deposit their eggs, female flies are capable of ranking the relative attractiveness of their options and choosing the &#34;greater of two goods.&#34; However, most egg-laying preference assays are not practical if one wants to take a systematic genetic screening approach to search for the circuit basis underlying this simple decision-making process, as they are population-based and laborious to set up. To increase the throughput of studying of egg-laying preferences of single females, we developed custom chambers that each can simultaneously assay egg-laying preferences of up to thirty individual flies as well as a protocol that ensures each female has a high egg-laying rate (so that their preference is readily discernable and more convincing). Our approach is simple to execute and produces very consistent results. Additionally, these chambers can be equipped with different attachments to allow video recording the egg-laying animals and to deliver light for optogenetics studies. This article provides the blueprints for fabricating these chambers and the procedure for preparing the flies to be assayed in these chambers.

High Throughput Assay to Examine Egg-Laying Preferences of Individual Drosophila melanogaster

This protocol describes a high throughput assay for testing egg-laying preferences of Drosophila melanogaster at single-animal resolution. This assay provides a simple, efficient, and scalable platform to identify genes and circuit components that control a simple decision-making process.

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For most animals, feeding is an essential behavior for securing survival, and it influences development, locomotion, health and reproduction. Ingestion of the right type and quantity of food therefore has a major influence on quality of life. Research on feeding behavior focuses on the underlying processes that ensure actual feeding and unravels the role of factors regulating internal energy homeostasis and the neuronal bases of decision-making. The model organism Drosophila melanogaster, with its great variety of genetically traceable tools for labeling and manipulating single neurons, allows mapping of neuronal networks and identification of molecular signaling cascades involved in the regulation of food intake. This report demonstrates the CApillary FEeder assay (CAFE) and shows how to measure food intake in a group of flies for time spans ranging from hours to days. This easy-to-use assay consists of glass capillaries filled with liquid food that flies can freely access and feed on. Food consumption in the assay is accurately determined using simple measurement tools. Herein we describe step-by-step the method from setup to successful execution of the CAFE assay, and provide practical examples to analyze the food intake of a group of flies under controlled conditions. The reader is guided through possible limitations of the assay, and advantages and disadvantages of the method compared to other feeding assays in D. melanogaster are evaluated.

The CApillary FEeder Assay Measures Food Intake in Drosophila melanogaster

The CApillary FEeder (CAFE) assay is a simple, budget-friendly, highly reliable method for investigating mechanisms underlying food intake. Used with the highly versatile genetic model organism Drosophila melanogaster, it provides a powerful means of gaining new insights into regulatory mechanisms of food intake.

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Despite decades of investigation, the neuronal and molecular bases of motivational states remain mysterious. We have recently developed a novel, reductionist, and scalable system for in-depth investigation of motivation using the mating drive of male Drosophila&#160;melanogaster (Drosophila), the methods for which we detail here. The behavioral paradigm centers on the finding that male mating drive decreases alongside fertility over the course of repeated copulations and recovers over ~3 d. In this system, the powerful neurogenetic tools available in the fly converge with the genetic accessibility and putative wiring diagram available for sexual behavior. This convergence allows rapid isolation and interrogation of small neuronal populations with specific motivational functions. Here we detail the design and execution of the satiety assay that is used to measure and alter courtship motivation in the male fly. Using this assay, we also demonstrate that low male mating drive can be overcome by stimulating dopaminergic neurons. The satiety assay is simple, affordable, and robust to influences of genetic background. We expect the satiety assay to generate many new insights into the neurobiology of motivational states.

Measuring and Altering Mating Drive in Male Drosophila melanogaster

This article describes a behavioral assay that uses male mating drive in Drosophila melanogaster to study motivation. Using this method, researchers can utilize advanced fly neurogenetic techniques to uncover the genetic, molecular, and cellular mechanisms that underlie this motivation.

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Quantification of Macronutrients Intake in a Thermogenetic Neuronal Screen using Drosophila Larvae

Foraging and feeding behaviors allow animals to access sources of energy and nutrients essential for their development, health, and fitness. Investigating the neuronal regulation of these behaviors is essential for the understanding of the physiological and molecular mechanisms underlying nutritional homeostasis. The use of genetically tractable animal models such as worms, flies, and fish greatly facilitates these types of studies. In the last decade, the fruit fly Drosophila melanogaster has been used as a powerful animal model by neurobiologists investigating the neuronal control of feeding and foraging behaviors. While undoubtedly valuable, most studies examine adult flies. Here, we describe a protocol that takes advantage of the simpler larval nervous system to investigate neuronal substrates controlling feeding behaviors when larvae are exposed to diets differing in their protein and carbohydrates content. Our methods are based on a quantitative colorimetric no-choice feeding assay, performed in the context of a neuronal thermogenetic-activation screen. As a read-out, the amount of food eaten by larvae over a 1 h interval was used when exposed to one of the three dye-labeled diets that differ in their protein to carbohydrates (P:C) ratios. The efficacy of this protocol is demonstrated in the context of a neurogenetic screen in larval Drosophila, by identifying candidate neuronal populations regulating the amount of food eaten in diets of different macronutrient quality. We were also able to classify and group the genotypes tested into phenotypic classes. Besides a brief review of the currently available methods in the literature, the advantages and limitations of these methods are discussed and, also, some suggestions are provided about how this protocol might be adapted to other specific experiments.

Quantification of Macronutrients Intake in a Thermogenetic Neuronal Screen using Drosophila Larvae

Described here is a protocol that enables the colorimetric quantification of the amount of food eaten within a defined interval of time by Drosophila melanogaster larvae exposed to diets of different macronutrient quality. These assays are conducted in the context of a neuronal thermogenetic screen.

Foraging and feeding behaviors allow animals to access sources of energy and nutrients essential for their development, health, and fitness. Investigating ...

Feeding Test: Assessment of Feeding Preferences in Drosophila melanogaster

Source: Bovier, T. F., et al. <a href="https://www.jove.com/video/59535/" target="_blank">Methods to Test Endocrine Disruption in Drosophila melanogaster</a>. J. Vis. Exp. (2019).
This video describes a feeding assay for fruit flies in which colored food is used to monitor feeding and the effect added compounds may have on feeding activity. The example protocol tests the effects of several endocrine disrupting chemicals (EDC).

Source: Bovier, T. F., et al. Methods to Test Endocrine Disruption in Drosophila melanogaster. J. Vis. Exp. (2019).
This video describes a feeding assay ...

A Simple Way to Measure Alterations in Reward-seeking Behavior Using Drosophila melanogaster

Summary

Explore More Videos

Chapters in this video

Combining Quantitative Food-intake Assays and Forcibly Activating Neurons to Study Appetite in Drosophila

Appetitive Associative Olfactory Learning in Drosophila Larvae

A Single-fly Assay for Foraging Behavior in Drosophila

Tracking Sugar-Elicited Local Searching Behavior in Drosophila

High-resolution Quantification of Odor-guided Behavior in Drosophila melanogaster Using the Flywalk Paradigm

High Throughput Assay to Examine Egg-Laying Preferences of Individual Drosophila melanogaster

The CApillary FEeder Assay Measures Food Intake in Drosophila melanogaster

Measuring and Altering Mating Drive in Male Drosophila melanogaster

Quantification of Macronutrients Intake in a Thermogenetic Neuronal Screen using Drosophila Larvae

Feeding Test: Assessment of Feeding Preferences in Drosophila melanogaster