Meal Duration as a Measure of Orofacial Nociceptive Responses in Rodents

Summary

A lengthening in meal duration represents orofacial nociceptive behavior in rodents similar to the guarding behavior of humans with orofacial pain. Eating is a behavior that requires no training or animal manipulation, requires cortical participation, and is not competing with other experimentally induced behaviors, distinguishing this assay from alternative reflex or operant measurements.

Abstract

A lengthening in meal duration can be used to measure an increase in orofacial mechanical hyperalgesia having similarities to the guarding behavior of humans with orofacial pain. To measure meal duration unrestrained rats are continuously kept in sound attenuated, computerized feeding modules for days to weeks to record feeding behavior. These sound-attenuated chambers are equipped with chow pellet dispensers. The dispenser has a pellet trough with a photobeam placed at the bottom of the trough and when a rodent removes a pellet from the feeder trough this beam is no longer blocked, signaling the computer to drop another pellet. The computer records the date and time when the pellets were taken from the trough and from this data the experimenter can calculate the meal parameters. When calculating meal parameters a meal was defined based on previous work and was set at 10 min (in other words when the animal does not eat for 10 min that would be the end of the animal's meal) also the minimum meal size was set at 3 pellets. The meal duration, meal number, food intake, meal size and inter-meal interval can then be calculated by the software for any time period that the operator desires. Of the feeding parameters that can be calculated meal duration has been shown to be a continuous noninvasive biological marker of orofacial nociception in male rats and mice and female rats. Meal duration measurements are quantitative, require no training or animal manipulation, require cortical participation, and do not compete with other experimentally induced behaviors. These factors distinguish this assay from other operant or reflex methods for recording orofacial nociception.

Introduction

Animal models have been used to study pain and nociception associated with orofacial damage and or inflammation^1,2, but a lack of appropriate animal models results in an incomplete understanding of the mechanisms. Although current models help us to understand various mechanisms involved in acute and chronic orofacial pain, there are strengths and weaknesses to these animal models.

Many models measure behavioral nociceptive responses for short durations. Face grooming is a known behavioral response following constriction of facial nerves³. Others studies measured facial rubbing with the ipsilateral fore or hindpaw, as well as, flinching of the head after administering formalin injections into the temporomandibular joint (TMJ) or lip^4-7. Head withdrawal latencies is another model for measuring nociceptive behavior where a modified tail flick analgesia meter is used to quantitate the nociceptive response (i.e. head withdrawal) after applying heat to the shaved vibrissae pad of a rat⁸. Digastric and masseter muscle activity has also been recorded as a correlate of pain after glutamate injections into the TMJ⁹. Another study has measured changes in sleep parameters to assess nociceptive responses in male and female rats with an inflamed TMJ, these parameters included sleep latency, rapid-eye-movement (REM), percentage of non-REM sleep, and percentage of REM sleep¹⁰. Most animal models that measure behavioral nociceptive responses utilize a short time frame, i.e. minutes to hours per day^11-14. In addition, most animal models testing occurs during the light phase and in a nocturnal animal, like a rat, this can cause stress which can confound the nociceptive results^15-18. The above assays measure nociceptive response in varying orofacial conditions but for short duration and hence can only be used to study acute disorders. An alternative assay has used facial expression as a measure of nociception of moderate duration, but this methodology can be subjective¹⁹.

To evaluate persistent or chronic orofacial nociception some have used the application of a von Frey filament on the surface of the skin to assess mechanical sensitivity of animals subjected to nerve constriction or TMJ inflammation^3,20. Liverman et al. 2009 measured withdrawal responses using graded monofilaments following CFA injections into the masseter muscle of rats ^21,22. Yamazaki et al. 2008 injected the TMJ with CFA and then over 14 days quantified nociceptive behaviors to mechanical or heat or cold stimulation applied over the TMJ region. Unfortunately, these nociceptive behavioral assays involve animal restraint, which produce stress hormones, learning or alternative behaviors that may interfere with the measured outcomes.

Models to measure nociception in teeth utilize the jaw opening reflex but this method can be unreliable²³ or imprecise²⁴. Electromyographic activity has been used to measure tooth nociception²⁵, but this method typically requires that the animal be unconscious, although in one study tooth nociception was investigated in freely moving rats²⁶. In 2008, Khan studied the relationship between dental nociception and masticatory function using a sensitive strain gauge²⁷ but this bite duration model requires restraining the animal from normal activity ²⁸. Bite force is a reliable measure of tooth pain in humans but because rats require training and/or restraint to measure bite force a source of stress is introduced which can produce findings with questionable physiological significance^29-31

Some limitations of restraint and stress can be overcome by using an operant design to assess nociceptive behaviors. One operant model uses avoidance of an uncomfortable temperature to evaluate and characterize orofacial nociception^32-35. This reward-conflict model is based on a reward of sweetened milk to induce the rodent to position its face voluntarily against a heated or cooled thermal probe^34,36. However, the test requires animal training, but a strength of the assay is the data is collected in an automated fashion. 

Still another animal model used nociception-induced gnawing dysfunction as an index of orofacial nociception³⁷. However, the rodent is confined to a tube and its only escape is to gnaw through a dowel to exit. An advantage of this model is that it measures jaw function after acute or chronic jaw injury in mice. However, the rodent is confined, which adds a confounding alternate competing behavior, i.e. escape, which would be stressful and thus could influence the nociception assay results.

Meal duration has been used to measure nociception in animals with TMJ arthritis^38-41, tooth pulp exposure⁴², and muscle damage⁴³. A rodent who experienced orofacial nociception ate more slowly after the animal initiated a meal. Patients experiencing TMJ pain also take longer to chew their food and the cycle length shortens when TMJ pain is diminished^44-46. The lengthening of meal duration when TMJ pain is present is expected to be a "guarding behavior", operationally defined as nociceptive behavior⁴⁷.

Meal duration measures TMJ nociception using a noninvasive method for up to 19 days in male and female rats and 6 days (longest period tested) in male mice and could be described as a biological marker of nociception^38-41. In support that meal duration measures nociceptive responses, nociception can be reduced by pharmacological intervention causing the animal's meal duration to return to normal^38,40,41. This was also confirmed when nociceptive neurons were destroyed using capsaicin; after nerve destruction the animals meal duration was not increased following injection of CFA into the TMJ 40.

Below is the protocol on how to obtain and statistically analyze meal duration data.

Protocol

In this model the rats or mice were given food and water ad libitum. The Texas A&M University Baylor College of Dentistry Institutional Animal Care and Use Committee approved all the experimental protocols. Below specific settings are shown in italics and are utilized specifically for the rat TMJ arthritis model. Mice can also be utilized in this model and alternative tooth pain and myogenic orofacial pain animal models can be used as well^42,43.

1. Software Settings

1. Load the Animal Monitor software for the feeder units onto the computer.
2. The Animals Monitor software is now opened by clicking on the icon and under the file menu selection choose the "configuration" pull down option.
3. In the "Animal Monitor Configuration" window uncheck the box entitled "Pellet Delivered Input" (Figure 1A).
   Note: This box is usually checked at the factory by default. Deselect this option. Once the investigator deselects this option the results are being recorded by removal of a pellet from the trough rather than when a pellet is being dispensed.
   Note: When the "Automatic File Naming" box is checked the software will automatically name the files (Figure 1A). This box is usually checked at the factory by default.
4. Set the timer lights to turn on at 06:00 (6:00 am) and to turn off at 20:00 (8:00 pm).
   Note: the hardware for the feeders units was modified so that the lights within the boxes are not controlled by the software but are wired instead to an isolated 24 hr timer. Thus, the "House Light" indicated on the configuration software was not functional in these examples.
5. Select the edit pull down menu and choose Experiment. A window with the title "Box 01 -" appears (Figure 1B).
6. Input the file name under which the data will be saved within this window.
   Note: if no file name is entered the data files will be automatically named by the software. Details of the experiment can be added in this window and saved with the data files. The information on the window can also be saved and used for subsequent experiments.
7. Enter a number greater than the total time of the experiment in the entry box entitled "Experiment Length (Days):".
   Note: This will ensure that the software saves the data until the experiment is complete, a mistake can be in setting this value too short, which will stop the software from recording the data even though animals are still in the feeding modules.
8. Enter 24 in the entry box entitled "Number of Hours in a Day".
   Note: the length can be modified to the experimenter's specifications.
9. Enter 10 in the box entitled "Meal Period End Criteria (min):"
   Note: for rats a meal was defined using a 10 min end of meal criterion based on previous studies⁴⁸ (i.e. a meal was bracketed before and after by a 10 min period of no pellets being taken) and the minimum meal size was set at three pellets per meal in this software package.
10. Enter 45 in the box entitled "Pellet Size (mg)". If an individual wanted to use mice input 20 within this window.
11. For rats add 45 mg rodent chow pellets to the feeder dispenser hopper.
    Note: for mice add 20 mg rodent chow pellets to the chow hopper.
12. In the "Phase" section of the Experiment window enter the term Day in the "Name" field and in the "# of Hours" field type 24 (Figure 1B).
    Note: below the "Phase" section there are two large open fields. The first large open field will be populated by the text entered in the previous "Phase" and "Name" fields.
13. The next large open field will have the "Day Phase" header Enter in the field entitled "Name" the word Light and enter in the field entitled "Percent" the number 60.
    Note: this entered text will populate the large field below.
14. Next enter in the field entitled "Name" the word Dark and enter in the field entitled "Percent" the number 40. Note: with these entries 60% of the day will be attributed to the light phase and 40% will be attributed to the dark phase. When the software calculates the meal patterns this information will be used. These settings typical for cycling female animals that are kept on a 14:10 light/dark cycle.
15. Select the "Set All Boxes Like This" button. Save this information and then hit OK.
16. The "Start Boxes" screen appears, select the feeders to activate and hit OK (Figure 1C).
17. Next the Animal Monitor Run-Time windows will appear with the meal pattern data (Figure 1D).
    Note: monitor and record the "# of Pellets Dispensed" from this window to determine the current health of the rat. A healthy male rat weighing around 300 g will typically eat between 300-800 45 mg pellets a day.
18. Files are generated daily and automatically saved that have a .CSV extension. Open these files to retrieve meal pattern data such as food intake, meal number, meal duration, meal size, or intermeal interval. The intervals for these meal patterns can be calculated for the entire day or for a phase of the day such as the Dark and Light phase. As noted above, the settings are for a 14:10 light/dark cycle. The raw data of when each pellet was removed from the trough is also recorded as a raw .CSV file.
    Note: In older versions of the software a minimum meal size of 3 pellets is not used in the calculations for generating the .CSV file.  Moreover, to get the average meal duration using the older software you must subtract 10 min from the values in the Average Meal Duration column of the .CSV file.
    When the software is operating the operator can manually select the file pull down menu option and daily select "save raw data". This will save the raw data for a 24 hr period rather than for the entire experiment. This raw data can be processed by alternative software at the user's discretion.
    Note: in the results shown we used alternative software to include a minimum meal size of 3 pellets.

2. Meal Duration Assay

1. Place individual rats in the sound-attenuated chambers equipped with photobeam computer-activated pellet feeders.
   Note: in these feeding units there are graduated water bottles and waste pans in which a sheet of thick absorbent paper is placed. In the feeder dispenser hopper 45 mg rodent chow pellets can be added for rats or 20 mg rodent chow pellets can be added for mice. Chow pellets are dispensed into a V shaped feeding trough and at the bottom of this trough is a photobeam. A pellet dispensed into the trough will be detected by breaking this photobeam. Once a rat removes this pellet from the feeder trough the photobeam is restored and this signals the computer to drop another pellet. Restoration of the photobeam also triggers the computer to record the date and time and keeps a running tally of the pellets dispensed. This tally of pellets is then analyzed to determine food intake, meal number, meal duration, meal size, or intermeal interval during any part of the day using Med Assoc. Inc. software. Again the raw .CSV data file can be analyzed by outside software^39,40,49-51.
2. Record the total number of pellets eaten, the amount of water consumed and the weight of the animals to discern the general health of the rats during the experimentation.
3. Rinse water bottles and fill with fresh water daily and add chow to the feeder hopper when needed.
4. Dump waste pan and the thick absorbent paper beneath the cage daily and blow the dust from moving part of the feeder daily using high pressure air.
   Note: personal protection equipment (e.g. gowns, gloves, masks, and masks) is required.
5. Remove floors, waste pans and water bottles after the experiment is completed and wash these components. Also, remove the feeding electronics from the caging wash by hand or in a dishwasher.

3. Induction of TMJ Arthritis

1. Place animals in the feeders at least 4 days before experimentation.
   Note: this data will be reported as predays to obtain a baseline feeding behavior. Then the animals are removed from the feeder for treatment. One type of treatment was to induce an arthritic TMJ. For this model rats are injected with complete Freund's adjuvant (CFA) at 08:00 (i.e. beginning of the light phase) after the rats are anesthetized with isoflurane (5% flow).
2. Inject 250 mg of CFA in 50 L bilaterally into the periarticular space of each TMJ.
   Note: in the example (Figure 2) 250 mg of CFA in 50 L was injected into each TMJ, but doses as low as 10 mg in volumes as small as 15 μl are effective over shorter periods of time⁵².
3. Inject control rats TMJ with 50 L of 0.9% saline. Note: all animals were mobile within 5 min or less after induction of anesthesia. In the event that a smaller dose of CFA is given in a lesser volume the control rats would receive this same volume of saline.

Results

Meal duration is a behavioral correlate of orofacial pain and meal duration measurements have been applied to animals with TMJ arthritis (Figure 2) and tooth decay (Figure 3). In one experiment, rats had TMJ arthritis after administering a high 250 mg dose of CFA and this treatment induced a significant increase in meal duration for 19 days (Figure 2). A lower dose of CFA (10 mg) injected into each TMJ joint produced a smaller increase in meal duration for only 2-3 days<...

Discussion

TMJ patients with orofacial pain report increased pain with increased chewing time, such that, the chewing cycle lengthens the longer the individual has been chewing^45,53-56. Our behavioral assay allows for similar testing in rats and mice when measuring meal duration³⁹. A recent unpublished study suggested that von Frey filament testing had greater sensitivity than meal duration measurements, showing a significant change for a longer period but von Frey filament testing can have a reflex response c...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Animal Monitor software	Med Assoc. Inc	SOF-710	East Fairfield, VT
Dustless Precision Pellets, Rodent, Grain-Based	Bio-Serv	F0165	45 mg pellets, 50,000/box
Dustless Precision Pellets, Rodent, Grain-Based	Bio-Serv	FO163	20 mg pellets
Complete Freund's Adjuvant	Chondrex, Inc.	7001	No loger provides the 5 mg/ml concentration.  Can use CFA from other sources as long as the investigator consistently uses this source