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Biology

Determining Basal Energy Expenditure and the Capacity of Thermogenic Adipocytes to Expend Energy in Obese Mice

doi: 10.3791/63066 Published: November 11, 2021
Michael Shum1, Zhiqiang Zhou2, Marc Liesa2,3,4

Abstract

Energy expenditure measurements are necessary to understand how changes in metabolism can lead to obesity. Basal energy expenditure can be determined in mice by measuring whole-body oxygen consumption, CO2 production, and physical activity using metabolic cages. Thermogenic brown/beige adipocytes (BA) contribute significantly to rodent energy expenditure, particularly at low ambient temperatures. Here, measurements of basal energy expenditure and total BA capacity to expend energy in obese mice are described in two detailed protocols: the first explaining how to set up the assay to measure basal energy expenditure using analysis of covariance (ANCOVA), a necessary analysis given that energy expenditure co-varies with body mass. The second protocol describes how to measure BA energy expenditure capacity in vivo in mice. This procedure involves anesthesia, needed to limit expenditure caused by physical activity, followed by the injection of beta3-adrenergic agonist, CL-316,243, which activates energy expenditure in BA. These two protocols and their limitations are described in sufficient detail to allow a successful first experiment.

Introduction

Metabolism can be defined as the integration of the biochemical reactions responsible for nutrient uptake, storage, transformation, and breakdown that cells use to grow and perform their functions. Metabolic reactions transform the energy contained in nutrients into a form that can be used by cells to synthesize new molecules and execute work. These biochemical reactions are inherently inefficient in transforming this energy into a usable form to sustain life1. Such inefficiency results in energy dissipation in the form of heat, with this heat production being used to quantify the Standard Metabolic Rate (SMR) of an organism1. The Standard condition was classically defined as heat production occurring in an awake but resting adult, not ingesting or digesting food, at thermoneutrality and without any stress1. The Basal Metabolic Rate (BMR) or basal energy expenditure in mice is referred to as the SMR but in individuals ingesting and digesting food under mild thermal stress (ambient temperatures 21-22 °C)1. The challenges and difficulties of directly measuring heat production made indirect calorimetry, namely calculating heat production from oxygen consumption measurements, to become the most popular approach to determine the BMR. Calculating the BMR from oxygen consumption is possible because the oxidation of nutrients by mitochondria to synthesize ATP is responsible for 72% of the total oxygen consumed in an organism, with 8% of total oxygen consumption also occurring in mitochondria but without generating ATP (uncoupled respiration)1. The majority of the remaining 20% of oxygen consumed can be attributed to nutrient oxidation in other subcellular locations (peroxisomal fatty acid oxidation), anabolic processes, and reactive oxygen species formation1. Thus, in 1907, Lusk established an equation, based on empirical measurements, widely used to transform oxygen consumption and CO2 production into energy dissipation as heat. In humans, the brain accounts for ~25% of the BMR, the musculoskeletal system for ~18.4%, the liver for ~20 %, the heart for ~10%, and the adipose tissue for ~3-7%2. In mice, the tissue contribution to BMR is slightly different, with the brain representing ~6.5%, the skeletal muscle ~13%, the liver ~52%, the heart ~3.7%, and adipose tissue ~5%3.

Remarkably, the biochemical reactions defining the BMR are not fixed and change in response to different needs, such as external work (physical activity), development (tissue growth), internal stresses (counteracting infections, injuries, tissue turnover), and changes in ambient temperature (cold defense)1. Some organisms actively recruit processes to generate heat in cold exposure, implying that heat produced by metabolism is not just an accidental byproduct. Instead, evolution selected regulatory mechanisms that could specifically upregulate heat production by changing the rate of metabolic reactions1. Thus, these same oxygen consumption measurements can be used to determine the capacity of an organism to generate heat in response to cold.

Two major processes contribute to heat generation upon cold exposure. The first one is shivering, which generates heat by increasing mitochondrial oxidative phosphorylation and glycolysis in muscle to cover the physical work done by involuntary muscle contraction. Therefore, cold exposure will increase oxygen consumption in muscles1. The second is Non-Shivering Thermogenesis, which occurs through an increase in oxygen consumption in brown and beige adipocytes (BA). Dissipation of energy into heat in BA is mediated by the mitochondrial uncoupling protein 1 (UCP1), which allows proton re-entry into the mitochondrial matrix, decreasing the mitochondrial proton gradient. The dissipation of the mitochondrial proton gradient by UCP1 increases heat production by the elevation in electron transfer and oxygen consumption and the energy released by proton dissipation per se without generating ATP (uncoupled). Moreover, thermogenic BA can recruit additional mechanisms that elevate oxygen consumption without causing a large dissipation in the proton gradient, by activating futile oxidative ATP synthesis and consumption cycles. The metabolic cages described here, namely the CLAMS-Oxymax system from Columbus Instruments, offer the possibility to measure energy expenditure at different ambient temperatures. However, to determine BA thermogenic capacity using whole-body oxygen consumption measurements, one needs to: (1) eliminate the contribution of shivering, and other non-BA metabolic processes to energy expenditure, and (2) specifically activate BA thermogenic activity in vivo. Thus, a second protocol describes how to selectively activate BA in vivo using pharmacology in anesthetized mice at thermoneutrality (30 °C), with anesthesia and thermoneutrality limiting other non-BA thermogenic processes (i.e., physical activity). The pharmacological strategy to activate BA is treating mice with the β3-adrenergic receptor agonist CL-316,246. The reason is that cold exposure promotes a sympathetic response releasing norepinephrine to activate β-adrenergic receptors in BA, which activates UCP1 and fat oxidation. Furthermore, β3-adrenergic receptor expression is highly enriched in adipose tissue in mice.

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Protocol

All experiments were approved by the Institutional Animal Care and Use Committee at the University of California, Los Angeles (UCLA). Mice were administered their diet and water ad libitum in the metabolic cage, housed in a temperature-controlled environment (~21-22 or 30 °C) with a 12h light/dark cycle. 8 week-old female mice fed a high-fat diet or chow diet for 8 weeks were used for this study.

1. Measurement of the Basal Metabolic Rate (BMR)

  1. Measure the total body weight of the mouse using a weight scale with accuracy in the range of 0.1 g.
    NOTE: This must be done before housing the mice in metabolic cages and after the 2-3 days of acclimation period to the metabolic cages.
  2. Measure the body composition, including fat and lean mass in non-anesthetized mice, using an appropriate body composition analysis system (see Table of Materials).
    NOTE: These measurements are needed to determine energy expenditure and are executed in parallel to total body weight measurements (step 1.1).
  3. Set up the metabolic cages and start the acclimation period.
    NOTE: The metabolic cages system includes an enclosure that allows the user to control the housing temperature and light of 12 cages (Figure 1A,B). Each cage has a water bottle, a feeder, and a grid (Figure 1C). The grid separates the mouse from the bottom of the cage, allowing feces collection. Once the cage is installed on each pre-determined space, a lid that seals the cage includes the water bottle slot, the tubing sampling air, the airflow system, and the physical activity sensor (Figure 1D).
    1. Turn on the temperature enclosure, the airflow system, and computer 2 h before starting the assay.
    2. After 2 h, open the software controlling the enclosure (see Table of Materials) and the airflow and let the software test the computer's communication with the equipment.
      NOTE: Oxymax software was used for the present work.
    3. Once communication is established, click File, then Open Experiment Configuration (Figure 2A) and select the experiment configuration predesigned by the vendor (or set up from a previous assay).
    4. Click on Experiment, then click on Properties, which will open the Experiment Properties window (Figure 2B).
    5. In the Properties window, set up the parameters of the environmental enclosure, including the Ambient Temperature (21 °C) and the 12 h Light cycles.
      NOTE: Keeping the software open and running allows air to flow into the cages and the enclosure to maintain the selected temperature and light cycles. Thus, the entire system can operate with mice inside the cages for several days, even without measuring oxygen and CO2.
    6. Click on Experiment, then click on Setup, and the Experiment Setup window will open, where the parameters of each metabolic cage are defined.
    7. Assign each mouse ID to the individual cage where the mouse is housed (Figure 2C).
    8. Include the lean mass or total body weight for each mouse only if no differences in body weight are observed between groups.
      NOTE: Obtaining raw values of oxygen consumption and energy expenditure facilitates ANCOVA analyses.
    9. Set the airflow rate to the metabolic cage at 0.5-0.6 L/min.
    10. On the Experiment Setup window, select the file saving path and name. Select the backup directory (Figure 2D).
    11. Add a pre-weighted amount of food to the feeders that covers at least food intake for 1 day.
      NOTE: If the cages have integrated scales, the food can be added directly, and the software will record it.
    12. Add the water bottles. Check that the bottle is sealed correctly and does not leak.
    13. 24 h after adding the food, weigh the food that is left on the cage.
      NOTE: The grams of food added minus the grams of food left will measure food intake.
    14. Start the oxygen, CO2, and activity measurements (step 1.4.10) once the food intake values are the same as those of mice housed in regular cages.
      NOTE: Here, the acclimation period (usually 2-3 days) is completed, and energy expenditure measurements can start.
  4. Indirect calorimetry and activity measurements to assess energy expenditure
    1. Measure the body weight, fat, and lean mass of all mice before starting the measurements.
      NOTE: These are the body weight and lean mass values used to perform ANCOVA analyses.
    2. Calibrate the CLAMS system's O2 and CO2 Zirconia-based detector (see Table of Materials) with the recommended oxygen concentration; always re-calibrate the detector before starting a new experiment.
    3. Use a calibration gas of known composition (20.50% oxygen and 0.50% CO2).
      NOTE: Gas suppliers often refer to this gas as "Primary Standard Grade."
    4. Turn on and ensure that the tank output pressure is at 5-10 psi.
    5. Open the Calibration Utility software for calibrating and testing the gas sensors (Figure 2E). Click on Experiment, then Calibrate.
    6. Press Start. Then, wait for the sensors to be tested and for the software to ask the user to turn the knobs of the gas sensor (Figure 2F) until the value of O2 identity is 1 (Figure 2G-H). Click Next when the step is complete.
      NOTE: If the Calibration Utility performs all current steps, the calibration will automatically proceed to the next step when the progress bar is filled.
    7. Verify the calibration results when all steps have been completed, and the results are presented.
    8. Turn off the calibration gas.
    9. Change food and add sufficient food for a 48-72 h period.
      NOTE: Although cages could be opened during the energy expenditure measurements to monitor the body weight and change the food daily, mice can be stressed by these manipulations, and measurements are lost when the cages are opened. Thus, it is recommended to avoid any manipulation during the measurement period.
    10. In the software, click on Experiment and then Run to start the oxygen, CO2, and activity measurements (Figure 3A).
      NOTE: The execution of the measurements can be tracked in real-time in a box located at the bottom left section of the software (red rectangle, Figure 3B). The red rectangle in Figure 3B shows that the system measures cage #1 at interval #3, namely the 3rd measurement. One measurement in one cage can take about 1 min. Thus, with 12 cages connected, oxygen consumption can be measured approximately every 12 min. Continuous measurements for a minimum of 48 h are recommended.
    11. Stop the experiment by clicking Experiment and then Stop (Figure 3C).
    12. Open the cages, weigh the mice and the food. Collect the feces to calculate the number of calories and lipids excreted over the 48-72 h measurements period.
      NOTE: Feces can be stored at -20 °C for later analyses. These cages cannot be effectively used to collect urine.
    13. Click on Experiments, then Export, and Export all subjects as a CSV file (Figure 3D).
      NOTE: To facilitate ANCOVA analyses, it is essential to export raw Oxygen consumption (VO2) and CO2 production (VCO2) values without being normalized by the body weight.
  5. Data analysis and quality control
    1. In the exported CSV sheet (Figure 3D) (from step 1.4.13), use the raw values of the oxygen consumption (VO2) and CO2 production (VCO2) measured every 12 min in the 2-3 day period that are automatically listed by the software and include a timestamp, namely the hour and date when they were measured.
      NOTE: VO2 and VCO2 values will be automatically corrected if body weight or lean mass values are added.
    2. In the exported CSV sheet, use the raw values of the respiratory exchange ratio (RER: VCO2/VO2) that are automatically calculated and listed by the software according to their timestamp.
      NOTE: Values close to 1 show that the mouse primarily oxidizes carbohydrates, while values closer to 0.7 represent that the mouse is mainly oxidizing fat. RER above 1 can occur during anaerobic exercise, as the body expels more CO2 to compensate for the acidosis caused by lactate. RER higher than 1 can indicate stress. The exported CSV file also contains the raw values from Energy expenditure (EE) or Heat production in calories per minute per mouse, measured every 12 min in the 2-3 days. Here, all the listed values include a timestamp.
    3. As single EE values per mouse are needed for an ANCOVA, average the EE values recorded between 09:00-16:00 for the light (day) phase and 19:00-04:00 for the dark (night) phase per mouse and day.
      NOTE: This can be done manually using Excel or Graph Pad. Selecting these two-time windows avoids averaging the intermediate, gradual, and unstable EE values associated with the light-dark phase transition.
    4. For a 48 h period, calculate the average of the two daylight values and the two dark phase values per mouse using Excel or Graph Pad.
    5. To quantify the total physical activity, use Excel or Graph Pad to sum the x, y, and z beam break counts measured in the metabolic cages and listed in the CSV file for each mouse.
      NOTE: The x,y,z total activity is calculated by doing first the average value of each X, Y, Z per mouse and cycle. Then, the sum of each average X, Y, Z values per mouse and cycle is determined to plot the data as in Figure 5E (being the average of 2 days).
    6. Alternatively, represent the data showing each measurement value over time, which generates curves that illustrate the changes in EE during the transition from light to dark cycles.
      ​NOTE: Please refer to the discussion section on how and when to perform ANCOVA analyses, and the different formulas used to calculate VO2, VCO2, and EE are provided in Supplementary File 1.

2. Measurement of the capacity of thermogenic adipocytes to expend energy

  1. Set up the measurements and mouse treatments. See step 1 for details on the experimental preparations to monitor oxygen consumption, as thermogenic capacity in adipocytes is determined indirectly by oxygen consumption following steps 2.1.1-2.2.2.
    NOTE: This protocol requires mouse anesthesia and acute treatment with the beta-3 receptor agonist CL-316,243 (see Table of Materials), giving a rapid assessment of BA thermogenic capacity.
    1. Perform body composition analysis and weigh the mice. Turn on the CLAMS, set up the temperature at 30 °C (thermoneutrality), and wait for 2 h for the whole system to warm up.
    2. Set up the rest of the assay conditions, including light, assign mouse ID to each cage and add body weight value of each mouse in the corresponding cage if no difference in body weight is observed between groups.
    3. Calibrate the oxygen/CO2 detector as in steps 1.4.2-1.4.7.
    4. Start the Experiment in the software.
    5. Inject each mouse with pentobarbital (60-120 mg/kg) and place each mouse in their assigned metabolic cage (step 2.1.2).
      NOTE: The dose of pentobarbital required to maintain mice asleep at thermoneutrality (30 °C) varies with the mouse strain and genotype. It is recommended to test different pentobarbital doses from 50 to 120 mg/kg and chose the one keeping the mouse anesthetized during 2-3 h at 30 °C. Efficient anesthesia is essential to remove the contribution of physical activity to energy expenditure.
    6. To ensure anesthesia, observe mice after pentobarbital injection until they are completely asleep and their decreased oxygen consumption rates become steady.
    7. Wait to obtain at least 3 stable consecutive oxygen consumption rates before injecting CL-316,243.
      NOTE: While waiting for the stabilization of oxygen consumption, prepare the syringes with CL-316,243 for each mouse (1 mg/kg).
    8. Open cage #1 and inject CL-316,243 subcutaneously immediately after one VO2 and VCO2 measurement occurred in cage #1. Return the mouse to cage #1 immediately after injection.
      NOTE: Measurements are being indicated in real-time in the bottom-left section of the software (Figure 3B, red rectangle).
    9. Wait for cage #2 to be measured (Figure 3B, red rectangle) and then proceed as in step 2.1.8 for cage #2.
      NOTE: Injecting CL-316,243 immediately after a measurement allows maintaining the time constant between injections. For instance, if there are 12 mice/cages running, with measurements collected in individual cages sequentially and the collection lasting 55 s per cage, then you should inject one mouse every minute. With these injection rates, the first measurement will occur after 12 min after injection in all 12 cages.
    10. Continue the energy expenditure measurements until the energy expenditure values plateau for 5-6 consecutive measurements, usually 90-180 min after injection.
      NOTE: Mice could wake up from the anesthesia during the experiments. These mice need to be removed from the analysis. Therefore, testing pentobarbital doses beforehand will increase the efficiency of the studies.
    11. Stop the energy expenditure measurements, but keep mice at their cages at 30 °C, until they wake up.
    12. After mice are fully awake, inspect the health of the mice and return them to their initial cages.
    13. Export the data of each mouse as a CSV file using the equipment software, as described in section 1.4.13.
  2. Data analysis
    NOTE: The data analysis was performed by Excel or Graphpad
    1. Plot the 3-5 consecutive values of VO2, VCO2, and EE that are stable and constant over time, as these are the values representing the metabolic rate when mice are fully anesthetized.
    2. Then, plot the first and the following consecutive VO2, VCO2, and EE measurements obtained after injection.
      NOTE: The absolute values of EE and the fold increase in EE induced by injection indicate BA thermogenic function7.

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Representative Results

Figure 4 shows VO2, VCO2, Heat production/Energy expenditure (EE), Respiratory Exchange Ratio (RER), and X, Y, Z physical activity values obtained using the metabolic cages of the CLAMS system. The VO2 and VCO2 provided by the CLAMS system is the volume of gas (mL) per minute and can be already divided by the body weight or the lean mass values by entering these weight values in the CLAMS software before starting the measurements. However, body weight values must not be entered if differences in body weight between groups of mice are observed, as ANCOVA analysis is needed and the Oxymax software cannot perform these calculations. The energy expenditure (heat) is calculated in kcal/h using the Lusk equation. Mice are nocturnal and spend more energy during the night/dark period, which means that energy expenditure calculations need to be separated according to the light cycle. As expected, mice during the dark phase have higher O2 consumption, CO2 production, and thus higher EE, as shown in Figure 4C. Mice on a regular diet and in the fed state, with food ingestion occurring in the dark cycle, are characterized by RER values close to 1 (Figure 4D), meaning a preference to use carbohydrates. During the light cycle, when mice mostly sleep and thus fast, there is a shift to fat oxidation, with RER values being closer to 0.7. Accordingly, physical activity, measured as x,y,z laser beam break counts, increases during the dark phase and decreases during the light phase (Figure 4E).

We compared 16 week-old female mice fed a high-fat diet (8 weeks) to chow-fed mice, allowing the comparison of energy expenditure between groups of mice with differences in body weight. As expected, high-fat diet feeding increases fat mass without changing the lean mass (Figure 5A-C). High-fat diet-fed mice ate more Kcal/day, mainly due to higher caloric density per gram of food (Figure 5D). In addition, physical activity was similar between chow, and high-fat diet-fed mice, even during the dark period (Figure 5E). The lower values of RER show the preference of high-fat diet-fed mice to use fat as the primary substrate for oxidation, as expected with higher fat intake and muscle insulin resistance (Figure 5F). Oxygen consumption increases in high-fat diet-fed mice, but not CO2 production (Figure 5G-H). The increase in oxygen consumption in high-fat diet-fed mice is accompanied by a significant increase in heat production/energy expenditure per mouse (Figure 5I). However, dividing energy expenditure by the lean mass of each mouse led to no differences in energy expenditure (Figure 5J), while dividing by total body weight showed a decrease in energy expenditure in high-fat diet-fed mice (Figure 5K). Cumulatively, these results indicate that dividing energy expenditure data by lean mass or total body weight can lead to opposite conclusions on the effects of high-fat diet feeding on energy expenditure. As suggested by multiple studies, the analysis of covariance (ANCOVA) allows determining whether differences in energy expenditure exist independently of the changes in body weight. To illustrate this point, an ANCOVA analysis was performed using the same data shown in Figure 5A-K, with energy expenditure being the dependent variable and body weight or lean mass as the covariates. While performing ANCOVA using total body weight as a covariate shows only a trend for high-fat diet-fed mice to have higher energy expenditure (Figure 5L), the high-fat diet-fed mice show a significant increase in energy expenditure when lean mass is used (Figure 5M). These data suggest that using total body weight to perform ANCOVA analyses could be underestimating energy expenditure4. The reasons can be that: (1) adipose tissue only contributes to ~5% of total energy expenditure and (2) the gain of fat mass induced by high-fat diet feeding results mainly from an expansion of triglyceride content in adipocytes, rather than from an increase in the number of oxidative thermogenic adipocytes.

Brown and beige adipocytes (BA) contribute to thermogenesis and consequently to energy expenditure in rodents. The contribution of BA to energy expenditure in vivo cannot be determined just by measuring whole-body oxygen consumption and calculating the BMR, as multiple tissues consume oxygen. The approach to determine BA thermogenic capacity in vivo involves anesthesia first, which is needed to limit oxygen consumption in all tissues. Then anesthesia is combined with a pharmacological approach to activate thermogenesis, mostly in thermogenic BA. As beta-3 adrenergic receptors are primarily expressed in adipose tissue, the beta-3 adrenergic agonist CL-316,243 can be used to activate BA thermogenic function. In addition, the anesthetized mice can be placed in a temperature-controlled enclosure at 30 °C, to prevent any uncontrolled sympathetic BA activation induced by ambient thermal stress. Figure 6 shows mice fed a high-fat diet anesthetized with pentobarbital and placed in the metabolic cages at 30 °C, to record energy expenditure at the sub-standard metabolic rate (Figure 6A-C,D). This measurement was followed by CL-316,243 injection, which raised oxygen consumption, CO2 production, and energy expenditure, as expected from BA activation (Figure 6A-C). A 2-3-fold increase in energy expenditure following beta-3 agonist treatment can be detected7.

Figure 1
Figure 1: The metabolic cages with the environmental enclosure and assembly of individual metabolic cages. (A) The metabolic cages in the environmental enclosure. (B) The enclosure can house 12 metabolic cages and allows controlling temperature and light. (C) Components of the metabolic cages before assembly. (D) Metabolic cages sealed with the lid. Please click here to view a larger version of this figure.

Figure 2
Figure 2: Experimental setup and calibration of the oxygen sensor. (A) A screenshot of the Oxymax software controlling the metabolic cages, showing selection and opening of an "Experimental configuration" window to set the (B) experimental properties, namely ambient light, and temperature. Then, the Experiment is configured using the (C) "Experimental Setup" window to assign a mouse ID, body weight, or lean mass to each cage, as well as the airflow rate for the 12 cages. (D) In the same "Experimental Setup" window, a file-saving path can be selected. (E) To calibrate the gas sensor, the user needs to turn the knob on the (F) gas detector to adjust the (G-H) O2 identity to 1. Please click here to view a larger version of this figure.

Figure 3
Figure 3: Start and stop of the measurements. (A) The Experiment is started by clicking on "Experiment," then "Run." (B) The users can see, real-time, which of the 12 cages is currently being measured (red rectangle), as well as a table with the measurements already collected. (C) The Experiment can be stopped by clicking on "Experiment," then "Stop." (D) The data can be exported to Excel by clicking on "File," then "Export," and then "Export all Subjects CSV." Please click here to view a larger version of this figure.

Figure 4
Figure 4: Metabolic parameters obtained. (A) Oxygen consumption.(B) CO2 production. (C) Energy Expenditure (EE) normalized to lean mass. (D) Respiratory exchange ratio (RER). (E) Physical Activity levels are calculated as the sum of X, Y, Z laser beam break counts. Data shows mean ± SEM. Student's t-test, **P < 0.01, ***P < 0.001. n = 7-8 female mice per group. Please click here to view a larger version of this figure.

Figure 5
Figure 5: The ANCOVA analysis allows appropriate interpretation of changes in energy expenditure in obese mice. (A-M) Measurements in female mice fed either a chow or high-fat diet (HFD) for 8 weeks. (A) Body weight. (B) Fat mass. (C) Lean mass. (D) Food intake. Student's t-test, ***P < 0.001. (E) Physical activity was assessed with the metabolic cages as counts of laser beam breaks in X, Y, Z. (F) The respiratory coefficient ratio (RER). (G) Oxygen consumption (VO2). (H) CO2 production (VCO2). (I) Energy expenditure (EE) was measured by indirect calorimetry. Energy expenditure was normalized to (J) Lean mass and (K) body weight. *P < 0.05 using Two-ANOVA. **P< 0.01, ***P< 0.001. (L) Covariate analysis (ANCOVA) of energy expenditure (EE) at night versus total body weight or (M) lean mass. Dashed lines represent the average body weight values modeled to determine VO2 and EE in each group. *P < 0.05 using ANCOVA. n = 7-8 female mice per group. Data shows mean ± SEM. Please click here to view a larger version of this figure.

Figure 6
Figure 6: The selective β3-agonist, CL-316,243 acutely increases energy expenditure in anesthetized mice at thermoneutrality. Female mice were anesthetized with pentobarbital (60 mg/kg) and placed in the metabolic cages set at 30 °C. Energy expenditure under anesthesia was recorded until 3 consecutive measurements showed the same values, reflecting complete anesthesia. The mouse from cage #1 was injected with CL-316,243 (1 mg/kg) immediately after an oxygen consumption measurement. The same injection approach was used in the other cages to ensure that the same time passed between injection and the first measurement in all mice. (A) Oxygen consumption. (B) CO2 production. (C) Energy expenditure. n = 4 female mice. Data shows mean ± SEM. Please click here to view a larger version of this figure.

Supplementary File 1: Formulas used by Oxymax software in the CLAMS system to calculate oxygen consumption, CO2 production, and energy expenditure. Please click here to download this File.

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Discussion

Indirect calorimetry has been used for years to assess whole-body energy expenditure4. This protocol described herein provides a straightforward method of measuring the basal metabolic rate and determining BA thermogenic capacity in vivo using metabolic cages.

The indirect calorimetry method described here confirms that dividing energy expenditure values by body weight values can be misleading. For example, it can conclude that energy expenditure is systematically lower in all mouse models with obesity. However, total energy expenditure can be higher in some mouse models of obesity, as in the case of an increase in food intake leading to obesity. Therefore, dividing energy expenditure by fat mass will always cause a misinterpretation of the process responsible for obesity in obese mice without primary defects in energy expenditure. In addition, dividing by lean mass is also inappropriate when changes in lean mass occur, as lean mass co-varies with energy expenditure, and energy expenditure can show a more significant decrease than any change in lean mass. This means that division of energy expenditure by body weight or lean mass can only be performed if no changes in body weight or body composition (i.e., lean mass and fat mass) are observed between the tested groups. As a consequence, the safest approach is to perform ANCOVA. This topic has been widely discussed in excellent articles, all of them concluding that an analysis of covariance (ANCOVA) is essential to compare energy expenditure between groups of mice with differences in total body weight or lean mass4,5. Here, SigmaPlot was used to perform ANCOVA analyses in-house, but many other advanced statistical analysis software can be used. The CalR website allows to upload data in one of their templates, but it might not always be possible depending on the experimental design5. Having statistical software to perform the ANCOVA "in-house" offers more flexibility on data analysis and presentation, but it is more time consuming6.

Thermoneutrality for mice is around 30 °C, which suppresses the activity of thermogenic brown and beige adipocytes (BA)1. Ambient temperature (21 °C) is below thermoneutrality, meaning that BA thermogenesis will contribute to energy expenditure in mice housed at 21 °C. So, the difference in energy expenditure between mice at ambient temperature vs. mice at thermoneutrality can be used to determine the contribution of BA to energy expenditure in a less invasive manner. However, this procedure requires the continuous use of the enclosure at 30 °C for 4 weeks, with thermoneutrality also causing differences in physical activity. In addition, thermoneutrality induces metabolic changes in other tissues, not just in BA. In a context where the main objective is to study changes in BA thermogenic capacity, the pharmacological approach described here has a list of advantages over housing mice at thermoneutrality over a long period.

Results are obtained in few hours, and the anesthesia suppresses the contribution of physical activity and other behavioral changes to energy expenditure. When assessing the effects of genetic manipulations in mice, metabolism might be changed in BA and other tissues. Thus, CL-316,243 treatment in anesthetized mice is the approach that can discern changes in BA activity with a higher dynamic range and specificity, with fewer confounders from energy expenditure stemming from other tissues. Alternatively, CL-316,243 can be injected in conscious mice as the system can measure physical activity. Therefore, if a change in physical activity occurs, it can be estimated and controlled5. In sum, while anesthesia can provide the highest dynamic range, measurements can be done without anesthesia if needed, as physical activity can be monitored.

When using the metabolic cages, caution must be taken regarding mice stress, and proper recovery is necessary. The social isolation of individual housing and the new environment of the metabolic cage stress the mice, resulting in decreased food intake and weight loss. Thus, food intake and body weight need to be monitored every 24 h. Mice recover normal food intake 48-72 h after placing them into the metabolic cage. As a result, calibration and oxygen consumption measurements start when food intake is recovered. Despite the metabolic cages system being on, calibration and measures are not performed during this acclimation period, as by definition, the BMR must be obtained in a stress-free mouse. Avoiding measurements during this period increases detector lifespan and reduces the use and consumption of Drierite (which traps water to prevent oxygen detector damage). Newer and more expensive systems used home-cage-based measurements, which diminishes stress.

ANCOVA analyses
An ANCOVA (analysis of covariance) is needed when comparing energy expenditure between two groups of mice with differences in body weight4. The reason is that an increase in lean mass will increase energy expenditure. ANCOVA tests whether energy expenditure is statistically significantly changed between groups, independent of differences in body weight and lean mass. ANCOVA achieves that by determining whether energy expenditure differed if both groups had the same body weight or lean mass. However, to calculate the energy expenditure at the same body weight/lean mass using ANCOVA, the correlation between the covariate (body weight/lean mass) and the variable (energy expenditure) must be similar between groups. The similarity of this correlation is tested using Levene's test for equality of variance5.

ANCOVA requires using more advanced statistical analysis software, such as SigmaPlot. Alternatively, different free websites can be used5. If ANCOVA shows that the effect observed between groups does not depend upon the value of the covariate (body weight/lean mass), the software will test whether the average of the variable (energy expenditure, VO2, VCO2) is different between the groups at a similar covariate (body weight/lean mass). The software will offer to make multiple comparisons with a suggested statistical test. If statistical significance is reached, it will confirm that the energy expenditure is significantly different between the two groups of mice at any given body weight value. The regression equation for the equal slopes model can be obtained from the analysis, which can be used in GraphPad or other graphical software to generate a graph for publication6.

Modifications and troubleshooting
The CLAMS system used in this protocol is constituted by small cages that are very different from the home cages that mice are used to, which include bedding. In addition, mice are social animals, and the need to house them individually, together with a new cage without bedding, causes initial stress to the mice. Thus, an acclimation of at least 2 days is necessary to allow mice to adapt to their new environments and mitigate stress. Usually, food intake comes back to what was recorded in their home cages on the third day. This acclimation period is unnecessary to assess BA capacity to expend energy, as it is performed in anesthetized mice.

Pentobarbital is a short-acting barbiturate that can be used as a sedative or anesthetic agent, but it is also used for euthanasia at higher doses. For an unknown reason, it was sometimes noticed that the efficacy of pentobarbital at 30 °C is different than at ambient temperature. Therefore, it is advised to test different pentobarbital doses in the mouse model at thermoneutrality. The main adverse effects of pentobarbital include respiratory depression and cardiovascular effects, such as reduced blood pressure, stroke volume, and hypotension8.

Limitations
Beta3-adrenergic receptors are expressed in adipose tissue and detectable in the myocardium, retina, gallbladder, brain, urinary bladder, and blood vessels9. As such, CL-316,243 can potentially increase energy expenditure in these other tissues where the receptor is expressed. However, it was demonstrated that most of the energy expenditure induced by CL-316,243 in control mice is UCP-1 dependent, a BA-specific protein10,11. It needs to be taken into consideration that some genetic modifications may exacerbate the actions of CL-316,243 in other tissues. In addition, the fraction of UCP1 independent respiration can still be driven by ATP-consuming futile cycles described in activated adipose tissue.

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Disclosures

The authors declare no conflict of interest to this protocol paper. M.L. is a co-founder and consultant for Enspire Bio LLC.

Acknowledgments

ML is funded by the Department of Medicine at UCLA, pilot grants from P30 DK 41301 (UCLA:DDRC NIH) and P30 DK063491 (UCSD-UCLA DERC).

Materials

Name Company Catalog Number Comments
CLAMS-Oxymax System Columbus Instruments CLAMS-center feeder-ENC Including enviromental enclosure and Zirconia oxygen sensor
Desktop PC with Oxymax Software HP/Columbus N/A PC needed to be purchased separately
Drierite jug (Calcium Sulfate with Cobalt Chloride Indicator) Fisher Scientific 23-116681 Needed to dry the gas entering the oxygen sensor, humidity can damage the sensor
NMR for body composition Echo-MRI Echo-MRI 100 Measure lean and fat mass in alive mice. It is necessary for ANCOVA analyses.
CL-316-243 Sigma C5976 Injected to the mice subcutaneously to activate thermogenesis
High fat diet Research Diets D12266B Provided to the mice prior and during measurements
Pentobarbital/Nembutal Pharmacy at DLAM N/A Anesthesia for the mice
Primary standard grade gas (tank and regulator) Praxair NI CD5000O6P-K/PRS 2012-2331-590 20.50% Oxygen, 0.50% CO2 balanced with nitrogen used for calibration

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References

  1. Rolfe, D. F., Brown, G. C. Cellular energy utilization and molecular origin of standard metabolic rate in mammals. Physiological Reviews. 77, (3), 731-758 (1997).
  2. Heymsfield, S. B., et al. Human energy expenditure: advances in organ-tissue prediction models. Obesity Reviews. 19, (9), 1177-1188 (2018).
  3. Kummitha, C. M., Kalhan, S. C., Saidel, G. M., Lai, N. Relating tissue/organ energy expenditure to metabolic fluxes in mouse and human: experimental data integrated with mathematical modeling. Physiological Reports. 2, (9), 12159 (2014).
  4. Tschop, M. H., et al. A guide to analysis of mouse energy metabolism. Nature. 9, (1), 57-63 (2011).
  5. Mina, A. I., et al. CalR: A Web-Based Analysis Tool for Indirect Calorimetry Experiments. Cell Metabolism. 28, (4), 656-666 (2018).
  6. Shum, M., et al. ABCB10 exports mitochondrial biliverdin, driving metabolic maladaptation in obesity. Science Translational Medicine. 13, (594), (2021).
  7. Assali, E. A., et al. NCLX prevents cell death during adrenergic activation of the brown adipose tissue. Nature Communication. 11, (1), 3347 (2020).
  8. Clark, J. D., Gebhart, G. F., Gonder, J. C., Keeling, M. E., Kohn, D. F. Special Report: The 1996 Guide for the Care and Use of Laboratory Animals. ILAR Journal. 38, (1), 41-48 (1997).
  9. Schena, G., Caplan, M. J. Everything You Always Wanted to Know about beta3-AR * (* But were afraid to ask). Cells. 8, (4), 357 (2019).
  10. Granneman, J. G., Burnazi, M., Zhu, Z., Schwamb, L. A. White adipose tissue contributes to UCP1-independent thermogenesis. American Journal of Physiology-Endocrinology and Metabolism. 285, (6), 1230-1236 (2003).
  11. Szentirmai, E., Kapas, L. The role of the brown adipose tissue in beta3-adrenergic receptor activation-induced sleep, metabolic and feeding responses. Scientific Reports. 7, (1), 958 (2017).
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Cite this Article

Shum, M., Zhou, Z., Liesa, M. Determining Basal Energy Expenditure and the Capacity of Thermogenic Adipocytes to Expend Energy in Obese Mice. J. Vis. Exp. (177), e63066, doi:10.3791/63066 (2021).More

Shum, M., Zhou, Z., Liesa, M. Determining Basal Energy Expenditure and the Capacity of Thermogenic Adipocytes to Expend Energy in Obese Mice. J. Vis. Exp. (177), e63066, doi:10.3791/63066 (2021).

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