A Method to Define the Effects of Environmental Enrichment on Colon Microbiome Biodiversity in a Mouse Colon Tumor Model

Summary

Environmental Enrichment (EE) is an animal housing environment that is used to reveal mechanisms that underlie the connections between lifestyle, stress, and disease. This protocol describes a procedure that uses a mouse model of colon tumorigenesis and EE to specifically define alterations in microbiota biodiversity that may impact animal mortality.

Abstract

Several recent studies have illustrated the beneficial effects of living in an enriched environment on improving human disease. In mice, environmental enrichment (EE) reduces tumorigenesis by activating the mouse immune system, or affects tumor bearing animal survival by stimulating the wound repair response, including improved microbiome diversity, in the tumor microenvironment. Provided here is a detailed procedure to assess the effects of environmental enrichment on the biodiversity of the microbiome in a mouse colon tumor model. Precautions regarding animal breeding and considerations for animal genotype and mouse colony integration are described, all of which ultimately affect microbial biodiversity. Heeding these precautions may allow more uniform microbiome transmission, and consequently will alleviate non-treatment dependent effects that can confound study findings. Further, in this procedure, microbiota changes are characterized using 16S rDNA sequencing of DNA isolated from stool collected from the distal colon following long-term environmental enrichment. Gut microbiota imbalance is associated with the pathogenesis of inflammatory bowel disease and colon cancer, but also of obesity and diabetes among others. Importantly, this protocol for EE and microbiome analysis can be utilized to study the role of microbiome pathogenesis across a variety of diseases where robust mouse models exist that can recapitulate human disease.

Introduction

Environmental enrichment (EE) studies utilize complex housing parameters to affect social stimulation (large housing cages, larger groups of animals), cognitive stimulation (huts, tunnels, nesting materials, platforms) and physical activity (running wheels). EE has been utilized by many labs to understand the effects of increased activity and improved social and cognitive interactions on disease initiation and progression using a wide array of mouse models, including barbering induced alopecia, Alzheimer's disease, Rett syndrome, and several tumor and digestive disease models^1,2,3,4,5,6.

Several mouse models have been developed to study colon tumorigenesis in mice. Perhaps the most well-defined model is the Apc^Min mouse. The Apc^Min mouse was developed in the laboratory of William Dove in 1990⁷, and has been used as a mouse model of mutations in the APC gene that are commonly associated with human colorectal cancer. In contrast to humans harboring APC mutations, Apc^Min mice primarily develop small intestinal tumors, with very rare occurrence of colon tumors. However, a Tcf4^Het allele with a single knockin-knockout heterozygous mutation in Tcf4, vastly increases colon tumorigenesis when combined with the Apc^Min allele⁸. Recently, this mouse model of colon tumorigenesis has been used to determine the effects of EE on colon tumorigenesis⁶. In the Bice et al. study, the physiological and phenotypic effects of EE on males and females of four different mouse lines (wild-type (WT), Tcf4^Het/+ Apc^+/+, Tcf4^+/+ Apc^Min/+, and Tcf4^Het/+Apc^Min/+)) were defined. Perhaps the most interesting finding was that EE significantly increases the lifespan of both male and female colon tumor-bearing animals. This demonstrated that EE may reduce at least some of the symptoms associated with colon tumorigenesis, and improve animal health. Remarkably, this improved lifespan in males is not a direct result of reduced tumorigenesis, and instead was linked to the initiation of a tumor wound healing response, including improved microbiome biodiversity⁶.

Several EE specific studies have been published with interesting results. However, from a technical standpoint, important results are often not translatable to other laboratories. Maintaining identical EE methodologies between different laboratories is an incredibly complex issue, not only due to enrichment devices and housing used, but also bedding, food, ventilation, breeding, genetics, activity in the room, and animal protocol requirements, among others^9,10,11. One example is animal integration, where animals must be stably integrated into the mouse colony, therefore normalizing genetic background and diet composition, to avoid non-treatment related effects. Further, many EE studies have been completed prior to the realization of the importance of the microbiome in disease, and the way that common mouse husbandry practices can affect the composition of the gut microbiome^10,12.

Breeding strategy and animal placement in EE can increase stress if not performed properly. Since EE studies utilize large numbers of both male and female animals and multiple genotypes, experimental setup can be difficult given the requirement for animals from several litters to be combined. Therefore, a breeding and weaning strategy was developed to allow for combining of weaned animals of the correct genotype from different litters. The primary rationale for this was to normalize the microbiota among litters and to reduce stress when animals were moved to the experimental environment. The microbiome was transmitted from the dam¹⁰. To provide microbial diversity to the colony, females were purchased from Jackson Labs and integrated into the colony for one month before the experiment began^9,10,12. To further normalize microbiome biodiversity between animals, females were co-housed prior to breeding. Following breeding, communal housing during rearing and the ability to escape nursing pups improved the stress levels of maternal care^13,14, possibly furthering microbiome normalization. To prevent non-EE related effects on the microbiome, this communal housing of all experimental animals prevented fighting and additional stress that occurred when combining several males from different litters into one experimental cage. Finally, equal numbers of animals of all genotypes were included in the cages. This provided the opportunity for improved microbiota biodiversity across genotypes, and removed the contribution of coprophagia (the animal's tendency to consume stool) or possible genotype-specific behavioral differences to the overall study.

This protocol provides a strategy that expands previous EE studies to include known aspects of microbiome research, including microbiota transmission and animal colony integration for microbiota normalization, to enable more uniform microbiome populations between experimental animals. Heeding these precautions is essential due to the ability of non-treatment related microbiota differences to confound study findings. Eliminating non-EE related microbiota changes will enable researchers to specifically define the role of EE on microbiota composition during disease development and progression.

Protocol

All methods described here were performed in accordance with protocols approved by the Institutional Animal Care and Use Committee (IACUC) at the University of Utah.

1. Experimental Design and EE and Control Cage Setup

Note: For reference, an outline of the experimental design is illustrated (Figure 1).

1. Set up control (NE) and EE cages (Figure 2).
   1. To set up NE cages, use autoclaved conventional control cages (Table 1) that lack enrichment devices.
   2. For large cages, drill one hole per cage that is large enough to accommodate a grommet and tunnel (Table of Materials).
   3. To set up pup rearing and EE cages, connect two large autoclaved cages with a sterilized grommet secured tunnel and 2 sterilized platforms to increase floor space (Table 1). For EE experiments, provide sterilized running wheels, tunnels, igloos, huts, crawl balls, and nesting material within the EE cages.
   4. Place both EE and NE cages in a ventilated rack to provide equal ventilation.
      Note: Two large cages with 2 platforms (Table 1) allow for a maximum of 12 pregnant females per pup rearing setup¹⁵ (see Table of Materials, step 3.2 in document, and Table 2).
   5. Feed mice ad libitum irradiated standard chow and autoclaved reverse osmosis water.
   6. Provide mice with sterile bedding materials.
      Note: All manipulations of empty cages and cages with animals must be done in the hood to prevent contamination. For cage manipulation of large cages, cover the hole in the cage with an adhesive film.
2. Prepare animals for breeding. Group house 15 2-month old females in a single large cage (Table 1) for 2 weeks prior to mating. Separately house 2-month old littermate males for 2 weeks prior to mating.
   Note: The number of females for breeding is dependent on the experiment and the number of animals required. In this study, 15 females were utilized to obtain 12 plugged females, which is the maximum number allowed in the pup rearing setup described in 1.1.2 (Table 2).
3. For breeding, combine sire and dam animals, 1 male per 2 females. The first check in the morning should be for vaginal plugs, which may be a visual sign that the animals have mated during the night.
   Note: House males and females together until each female has plugged. A vaginal plug can be identified visually, if it is external.
   1. To detect internalized plugs, a probe is inserted into the vaginal opening and if the vaginal plug is present, the probe is not easily inserted (¹⁶; see section 4.3.6).
      Note: Record the morning a plug is detected as ½ day, since the mating occurred in the night.
   2. Once females have vaginal plugs, transfer them to a large pup rearing cage for group housing with other mated females (Setup in step 1.1.2 without enrichment devices).
   3. Replace mated females with new unmated group housed females for mating and continue mating to obtain a maximum number of litters in a 7-day period.
      Note: All animals must have a delivery date within 7 days of each other.
4. Allow pregnant females to give birth in group housing so that all litters are raised within one large pup rearing cage (Setup in step 1.1.2 without enrichment devices).
   1. Keep track of pup numbers and birthdates, and begin genotyping pups at 7 days of age.
      1. Tattoo pups on their toes at 7 days of age with a number code to identify them^13,17.
      2. Clean the toe with 70% ethanol and gently insert a micro-tattoo device containing ink into the skin surface parallel to the toe¹⁷ (see Table of Materials).
      3. Collect tissue with scissors for genotyping from the tail tips by incising a small piece of tissue from 7-day old neonates.
   2. Isolate genomic DNA from tissue and perform PCR using a conventional HotSHOT method as described in ¹⁸.
   3. Separate animals by sex at 14-21 days into large cages with mothers.
      Note: Ensure that the older pups are able to feed on their own, and that younger pups continue to nurse until old enough to feed on their own.
   4. At 21-28 days, distribute male and female animals separately by genotype into NE or EE environments, making sure to keep equal proportions of each genotype per cage (Figure 2A).
      Note: Ensure that the total number of animals allowed in each NE or EE cage is based on the maximum number allowed by IACUC (Table 2). The NE cages have at most 5 animals (Table 2). In EE cages, for social stimulation, no fewer than 20, and with space restrictions, no more than 41 animals should be allowed in the EE cage (Table 2).

2. Stool Collection at 16 Weeks of Age

1. Begin stool collection 1 to 2 days prior to sacrifice, and separately collect stool on the day of sacrifice during dissection using sterile tools.
   Note: Collecting stool at the same time 1-2 days prior to collection may help to avoid the loss of a sample due to the possibility that no stool is present at the time of collection.
   1. To collect stool from live animals, carefully scruff the animal over a clean cage. Collect stool using sterile forceps into a sterile microfuge tube.
      Note: Animals will typically eliminate stool when immobilized, which allows for rapid stool collection directly into a sterile microfuge tube. If an animal does not immediately defecate when immobilized, place it into a clean cage and wait for the animal to defecate (typically up to 1 h).
   2. Collect stool on the day of sacrifice.
      1. For euthanizing the animal, place the animal in a bell jar containing a small container with a cotton ball soaked in isoflurane. Once cessation of breathing is observed (usually after 2 min), lay the animal on its back to allow colon dissection.
      2. Apply 70% ethanol to the mouse abdomen.
      3. Lift the skin anterior to the urethral opening with forceps, and use scissors to cut along the ventral midline until reaching the ribcage, and cut from the base of the first incision towards each leg. Fold back the skin and use scissors to cut through the peritoneal wall in the same pattern.
      4. Use forceps to grasp the distal colon at the anus to dissect and detach the distal colon from the rectum. While pulling the colon vertically with forceps, use scissors to cut through the mesentery to release the colon.
      5. Cut the colon just below the cecum and lay it on filter paper. Use forceps to lift the top of the colon tube, opening the lumen to allow one side of open scissors to be inserted. Cut longitudinally, distal to proximal, and splay open the colon lengthwise.
      6. Collect stool from the distal colon into a sterile microfuge tube using sterile forceps.
2. Store stool in a microfuge tube at -80 ˚C until time of bacterial DNA isolation.
   Note: On the day of sacrifice, in addition to the stool, collect other samples such as whole blood, serum, plasma, normal and tumor tissue from colon and small intestine, microsomes, adipose tissue, etc. to address defined questions in the study.

3. Genomic DNA Isolation from Stool

Note: Utilize a commercial kit to isolate microbial DNA from stool following a stool pathogen detection protocol. Remove samples directly for the -80 ˚C freezer and store on dry ice while weighing.

1. Transfer up to 220 mg of stool to a clean microfuge tube containing 1.4 mL of room temperature (RT) stool lysis buffer (see Table of Materials).
2. Vortex sample for 1 min to thoroughly homogenize solids (Figure 2B). Heat the suspension to 95 ˚C for 5 min to lyse all bacteria (including Gram-positive bacteria).
3. Vortex samples for 15 s and then centrifuge at 20,000 x g for 1 min to pellet the stool solids. Transfer supernatant to a 2-mL microfuge tube. Add one tablet to each sample to absorb PCR inhibitors, vortex until the tablet is dissolved, and incubate the sample at RT for 1 min.
4. Centrifuge the sample at 20,000 x g for 3 min and transfer the supernatant to a new microfuge tube. Centrifuge at 20,000 x g for 3 min. Aliquot 15 μL of proteinase K (20 mg/mL stock) into a new 1.5 mL microfuge tube. Pipette 200 μL of the sample into the tube containing proteinase K.
5. Add 200 μL of guanidinium chloride lysis buffer to the tube, vortex thoroughly for 15 s (see Table of Materials) and incubate the sample at 70 ˚C for 10 min. Add 200 μL of ethanol (96-100%) to the tubes and mix well by vortexing.
6. Place a silica based spin column in a 2-mL collection tube and apply the samples to the column. Close the lid and centrifuge for 1 min at 20,000 x g.
7. Transfer the column to a new 2 mL collection tube and add 500 μL of wash buffer 1 to the column, cap the column and centrifuge for 1 min at 20,000 x g. Transfer the column to a new 2 mL collection tube and add 500 μL of wash buffer 2 to the column, close the cap and centrifuge at 20,000 x g for 3 min.
8. With the cap closed, transfer the column to a new 2 mL collection tube, and centrifuge for an additional 1 min at 20,000 x g to remove residual wash buffer. Transfer the column to a 1.5 mL labeled microfuge tube and elute sample by adding 200 μL of elution buffer containing EDTA to the membrane (see Table of Materials).
9. Close the cap and incubate at RT for 1 min. Centrifuge the sample for 1 min at 20,000 x g. Discard the column.

4. DNA Concentration Determination and Sample Preparation for PCR

Note: Utilize a fluorometer and a commercially available dsDNA fluorescent assay to determine genomic DNA concentration in each sample (see Table of Materials). The fluorescent dye must bind double stranded DNA specifically.

1. Prepare a 1:200 dilution of each sample (1 µL of each sample in 199 µL dsDNA master mix) and a 1:50 dilution of standards. Analyze on a fluorometer using the dsDNA setting.
   Note: A high volume of DNA in PCR can be inhibitory, therefore, the volume of DNA used must not be more than 10% of the final volume of the PCR. A fluorometer enables accurate measurement of DNA in the sample, as only DNA bound to the fluorescent dye will fluoresce, eliminating the possible contribution of contaminants to the final calculated DNA concentration. This level of accurate quantitation is essential for the downstream sequencing application.
2. Prepare PCR templates diluted to 5 ng/μL with the appropriate volume of 10 mM Tris, pH 8.5 to make working template stocks of each sample.
3. Store samples at -20 °C.

5. Design Primers to the 16S Desired V Regions

1. Design primers to selectively amplify the desired V 16S rRNA regions.
2. Analyze primers with Probe Match, from the Ribosomal Database Project¹⁹, to determine the approximate hit rate for various phyla.
   Note: For V1-V3 regions, the current study used published primers Bosshard forward²⁰, which bind at position 8 within the V1 region, and 533 reverse²¹, which binds at position 533 within the V3 region. Primers must include overhang adapter sequences for indexing.
3. When designing primers, include adapter sequences at the 5' ends of each primer, as recommended for 16S metagenomics sequencing library preparation²² (Table 3).
4. Synthesize these large primers with cartridge purification. Reconstitute desiccated primers and dilute a PCR working stock to 1 μM in 10 mM Tris, pH 8.5.

6. Amplicon PCR to Amplify the V Region(s) with Overhang Adapter Sequences Attached ²²

1. Set up the amplicon PCR reaction mix as described in Table 4.
2. Place an adhesive clear PCR plate seal on the plate and run the amplicon PCR using the parameters in Table 5.
3. (Optional) Run amplicon PCR products on an agarose gel or a high sensitivity DNA assay that enables quantitative measurement of amplicon size (see Table of Materials).
   Note: The amplicon size from this study is 550 bp (Figure 3A).

7. PCR Cleanup Using Magnetic Beads ²²

1. Centrifuge the amplicon PCR plate quickly at 1,000 x g for 1 min to collect condensation.
   Note: PCR tube strips can be used instead of PCR plates to minimize contamination. Discard tube lids and never reuse.
2. Vortex the magnetic beads to evenly disperse them, and add 20 μL of magnetic beads to each amplicon PCR well, then pipette the entire volume up and down slowly 10 times.
3. Incubate at RT for 5 min. Place the PCR plate on a magnetic stand for 2 min until magnetic beads are collected and the supernatant is clear. Remove and discard the supernatant.
4. Wash beads with 200 μL fresh 80% ethanol while the PCR plate is on the magnetic stand and incubate for 30 s at RT on the magnetic stand. Carefully remove the supernatant.
5. Repeat the wash for a second time. Now, use a fine pipette tip to remove any residual ethanol from the wells and allow air drying for 10 min.
6. Remove the PCR plate from the magnetic stand and add 52.5 μL of 10 mM Tris pH 8.5 to each well. Pipette up and down 10 times to suspend beads and incubate at room temperature for 2 min.
7. Transfer the PCR plate to the magnetic stand to collect magnetic beads and transfer 50 μL of the supernatant to a clean PCR plate. Place an adhesive clear PCR plate seal on the plate and store at -20 ˚C for up to one week.

8. Preparation of a Plate Scheme for Index PCR

Note: To generate a V1-V3 library, a second PCR was performed with an index kit (see Table of Materials). A default indexing scheme was used to map out unique dual index combinations for each sample (Figure 3B and ²³).

1. Ensure that each sample has a unique combination of 2 index primers (i.e., dual indexing).

9. Perform Index PCR to Attach Barcodes to the Adaptor Sequences as Described ²² .

1. Transfer 2.5 μL of PCR amplicons (clean amplicons) to a new 96 well plate and place in an index plate fixture to aid in indexing.
2. Arrange the index 1 and index 2 primers as in the example of the prepared plate graphic (Figure 3B).
   Note: Visual cues are provided to avoid primer mix-ups: index 2 primer tubes should have white caps and clear solution, while index 1 primer tubes should have orange caps and yellow solution.
3. Assemble the index PCR Mix reaction as described in Table 6. Mix by pipetting up and down 10 times.Cover with an adhesive clear PCR plate seal and centrifuge to collect at 1,000 x g at room temperature for 1 min.
4. Run the index PCR using the parameters in Table 7.

10. Purify Final PCR Library

Note: This PCR clean-up is identical to step 7 above, and uses magnetic beads to perform PCR Clean-Up of the index PCR²².

1. Centrifuge the PCR plate from step 10 quickly at 1,000 x g for 1 min to collect condensation.
2. Vortex the magnetic beads to evenly disperse them, then add 20 μL of magnetic beads to each amplicon PCR well, then pipette the entire volume up and down slowly 10 times to mix.
3. Incubate at RT for 5 min.
4. Place PCR plate on a magnetic stand for 2 min until magnetic beads are collected and supernatant is clear. Remove and discard the supernatant.
5. Wash beads with 200 μL fresh 80% ethanol while the PCR plate is on the magnetic stand and incubate for 30 s at room temperature on the magnetic stand. Carefully remove the supernatant.
6. Repeat the wash for a second time.
7. Following the second wash, use a fine pipette tip to remove any residual ethanol from the wells and allow air drying for 10 min.
8. Remove the PCR plate from the magnetic stand and add 52.5 μL of 10 mM Tris pH 8.5 to each well. Pipette up and down 10 times to suspend beads and incubate at room temperature for 2 min.
9. Transfer the PCR plate to the magnetic stand to collect magnetic beads and transfer 50 μL of the supernatant to a clean PCR plate. Place an adhesive clear PCR plate seal on the plate and store at -20 ˚C for up to one week.
10. (Optional) Run index PCR products on an agarose gel or a high sensitivity DNA assay that enables quantitative measurement of amplicon size (see Table of Materials).
    Note: The final indexed library size from this study was 668 bp (Figure 3C-D).

11. Quantify, Normalize, and Pool the Indexed Libraries for Sequencing

1. Determine the DNA concentration of each sample with a fluorometer and a dsDNA fluorescent assay kit (see Table of Materials).
   1. Prepare a 1:200 dilution of the sample (1 µL of each sample in 199 µL dsDNA master mix, which includes buffer and reagent) for each of the indexed samples and standards (190 µL dsDNA master mix and 10 µL of standard). Analyze on a fluorometer using the dsDNA setting.
2. Following the DNA concentration calculation, normalize the libraries by calculating the average library size. Do this by summing adapter lengths, index lengths, and V amplicon size from primers, and view products by agarose gel to be certain the actual size is similar to the calculated size (Figure 3C, see ²²).
   1. Alternatively, utilize a high sensitivity DNA assay that enables quantitative measurement of DNA integrity, amplicon size, and concentration (Table of Materials, Figure 3D).
      Note: In this study, the average library size was calculated based on summing adapter lengths, index lengths, and V1-V3 amplicon size from primers. The average size was 668 bp.
   2. Concentrations of samples are normalized using the formula in Table 8.
3. Dilute samples to 4 nM and pool 5 μL from each 4-nM sample into a single tube for sequencing.

12. Sequence the Library using a Next Generation Sequencing System and Parse the Data

1. Sequence the library.
   Note: For this study, the University of Utah High Throughput Genomics Core performed library denaturation and sample sequencing (as described in ^6,22).
2. Parse the data.
   Note: To separate data from pooled samples, index reads were identified and separated (as described in ²²).
3. Generate FASTQ files and utilize this for subsequent data analysis.

13. Analyze Sequenced Data from the 16S Amplicon Library

Note: This step is performed as described in Bice et al., 2017⁶.

1. Install freely available data analysis tools (see Table of Materials;²⁴).
2. Assemble demultiplexed fastq files from the sequenced data (as described in^25,26). Discard all unassembled sequences.
3. Perform analyses following a de novo open taxonomic unit (OTU) picking protocol (as described in ²⁷).
   1. Bin sequences into a single fastq file by sampleID and group sequences with 97% or greater similarity into OTUs, as described in ²⁸. Align representative sequences of core set with minimum sequence length of 150 and 75% percent identity^29,30. Assign taxonomy as described²⁸.
      Note: Samples can be binned and analyzed³¹, followed by taxonomic assignment and OTU table construction³².
   2. Create a mapping file that identifies descriptive names and characteristics of samples to link to sample identification and validate the mapping file^33,34.
   3. Make an OTU network that links OTUs to sample descriptions using a mapping file³⁵.
   4. Calculate taxonomy summaries in terms of relative abundance by summarizing taxa through plots³⁶.
   5. Explore alpha diversity of samples at uniform sequencing depth appropriate to samples. To define the appropriate depth for alpha diversity, summarize total counts observed in each sample by using the biome summarize-table command, as described in ³⁷.

Results

Several studies have demonstrated that the practice of mind-body medicine improves health outcomes. Similarly, in mice, environmental enrichment improves outcomes including improved lifespan and tumor wound repair⁶. Therefore, an EE procedure was developed with the aim of defining the role of microbiota in this phenotype while first normalizing the microbiome prior to the initiation of the experiment (Figure 1). Importantly, all breedi...

Discussion

This procedure allows for the analysis of microbiota isolated from stool following environmental enrichment of normal or tumor bearing animals. Because these are large experiments which involve breeding to obtain many animals of different sexes and genotypes, normalizing the microbiome between animals prior to commencement of the experiment is essential to avoid non-EE related effects on microbiome biodiversity.

For consistency between NE and EE conditions, the breeding process is conducted to...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Teklad Diets/Harlan Labs Chow	Harlan Labs	3980X	Standard irradiated chow formulated by Dr. Mario Capecchi in collaboration with Harlan Labs.
Cell-Sorb Plus bedding	Fangman Specialties	82010	Autoclave prior to use.
AIMS Tattooing System For Neonates	AIMS	NEO-9	https://animalid.com/neonate-rodent-tattoo-identification/32. Other animal grade tattoo systems and inks can be used with similar results including the Aramis Micro Tattoo Kit.
Zyfone One Cage 2100 AllerZone Mouse Micro-Isolator System Complete with cage, AllerZone filter top and modular diet delivery system	Lab Products	82120ZF	Each EE cage requires one of each catalog # 82120ZF, 82100ZF, and 82101ZF, as well as two of 82109ZF. Food is only in one side.
Zyfone One Cage 2100 Life Span Enrichment Device	Lab Products	82109ZF	Each EE cage requires one of each catalog # 82120ZF, 82100ZF, and 82101ZF, as well as two of 82109ZF. Food is only in one side.
Zyfone One Cage 2100 Cage 13-7/8" Length X 19-1/16" Width X 7-3/4" Depth	Lab Products	82100ZF	Each EE cage requires one of each catalog # 82120ZF, 82100ZF, and 82101ZF, as well as two of 82109ZF. Food is only in one side.
Zyfone One Cage 2100 AllerZone Micro-Isolator filter top	Lab Products	82101ZF	Each EE cage requires one of each catalog # 82120ZF, 82100ZF, and 82101ZF, as well as two of 82109ZF. Food is only in one side.
Tunnel	Bio-Serv	K3323 or K3332	Connect cages together and use for enrichment
Grommet to connect Tunnel to cages	Fabricated by the University of Utah Machine Shop	n/a	Be certain the material is resistant to chewing and autoclavable
Fast-track wheel	Bio-Serv	K3250 or K3251	Use with mouse igloo and floor
Mouse Igloo	Bio-Serv	K3328, K3570 or K3327	Use with Fast-track wheel and floor
Mouse Igloo floor	Bio-Serv	K3244	Use with mouse Igloo and Fast-Track
Mouse Hut	Bio-Serv	K3272, K3102 or K3271
Crawl Ball	Bio-Serv	K3330 or K3329
Bio-hut	Bio-Serv	K3352	Wood pulp hut used for sheltering and nesting
Adhesive film	VWR	60941-072	Use to temporarily cover drilled hole in large cage to prevent mice from escaping
Laminar Flow Ventilated Rack	Techniplast	Bio-C36	The cabinet we used in this study is not currently supplied. The Bio-C36 is very similar.
1.5 mL Microfuge Tube- RNAse and DNAse free	Any supplier
QIAamp DNA Stool MiniKit	Qiagen	51504	This kit supplies reagents for 50 DNA preparations. Stool Lysis Buffer=ASL; Guanidinium Chloride Lysis Buffer= AL; Wash Buffer 1 with Guanidinium Chloride= AW1; Wash Buffer 2= AW2; Elution Buffer with EDTA=AE
Waterbath (capable of heating to 95)	Any supplier		For 94 degree incubation of stool samples to lyse cells.
Waterbath (capable of heating to 70 degrees)	Any supplier		For 70 degree incubation of stool samples
Ethanol (200 proof)	Sigma Aldrich	E7023
Fluorometer: Qubit	ThermoFisher Scientific	Q33216
Qubit dsDNA broad Range Assay Kit	ThermoFisher Scientific	Q32850
EB Buffer or 10 mM Tris pH 8.5	Qiagen	19086
Experiment specific primers	Any Supplier
PCR grade water	Any supplier
2X KAPA HiFi HotStart Ready Mix	Kapa Biosystems	KK2601	For Amplicon Amplification (1.25 mL allows 100 rxns).
Agarose for running diagnostic gels	Any supplier
TapeStation High Sensitivity D1000 Screen Tape Trace	Agilent	5067-5583	TapeStation or Bioanalyzer instruments are common in Institutional Genomics Cores to analyze library quality . Alternatively a Bioanalyzer DNA1000 Chip (Agilent, 5067-1504) can be used.
Agencourt AMPure XP Magnetic Beads	Beckman Coulter	A63880	Magentic beads For PCR cleanup- 5 mL will clean 250 PCR reactions
Magnetic stand	Life Technologies	AM10027
Library Preparation Guide	Illumina		Illumina. 16S Metagenomic Sequencing Library Preparation: Preparing 16S ribosomal RNA Gene Amplicons for the Illumina MiSeq System. https://support.illumina.com/content/dam/illumina-support/documents/documentation/chemistry_documentation/16s/16s-metagenomic-library-prep-guide-15044223-b.pdf.
Unique Dual Indexing	Illumina	Illumina Experiment Manager Software	Freely available at: https://support.illumina.com/sequencing/sequencing_software/experiment_manager/downloads.html
Nextera XT 96 Index Kit	Illumina	FC-131-1002	Used to add barcodes to amplicons
MicroAmp Optical 96-well reaction plate	Applied Biosystems/ThermoFisher	N8010560
TruSeq Index Plate Fixture	Illumina	FC-130-1005
Adhesive clear plate seal	Applied Biosystems /ThermoFisher	4360954	Applied Biosystems/ThermoFisher Microamp adhesive film
Sequencing by MiSeq with v3 reagents and dual 300 bp reads	Illumina	MS-102-3003
PhiX Control Kit	Illumina	FC-110-3001
Proteinase K (600 mAU/ml)	Qiagen	19131	Equivalent to 20 mg/ml of proteinase K. Supplied with QiaAmp kit
Data Analysis Tools	Qiime	QIIME software Tools	Installation may differ based on your system and the QIIME website describes several options (http://qiime.org/install/install.html). For this study, MacQIIME software package 1.9.1 was utilized (compiled by Werner Lab, SUNY, http://www.wernerlab.org/software/macqiime
Step 13.2.	Qiime	FastQ Join method	(http://code.google.com/p/ea-utils  ).  For this study Multiple join paired ends was used http://qiime.org/scripts/multiple_join_paired_ends.html. Aronesty, E. ea-utils: Command-line tools for processing biological sequencing data. Expression Analysis, Durham, NC. (2011).
Step 13.3.	Qiime	De-Novo OTU picking protocol	http://qiime.org/scripts/pick_de_novo_otus.html.
Step 13.3.1.		Open Taxonomic Units (OTUs) using Uclust	Edgar, R.C. Search and clustering orders of magnitude faster than BLAST. Bioinformatics. 26 (19), 2460-2461, doi:10.1093/bioinformatics/btq461 (2010).
Step 13.3.1.	Pynast	Pynast	Caporaso, J.G. et al. PyNAST: a flexible tool for aligning sequences to a template alignment. Bioinformatics. 26 (2), 266-267, doi:10.1093/bioinformatics/btp636 (2010).
Step 13.3.1.	Pynast	Pynast_Greengenes	DeSantis, T.Z. et al. Greengenes, a chimera-checked 16S rRNA gene database and workbench compatible with ARB. Appl Environ Microbiol. 72 (7), 5069-5072, doi:10.1128/AEM.03006-05 (2006). Greengenes version 13_8 was used in this study
13.3.1. Note:	Qiime	Multiple Split Libraries	http://qiime.org/scripts/multiple_split_libraries_fastq.html.
13.3.1. Note:	Qiime	Pick de novo OTUs script	http://qiime.org/scripts/pick_de_novo_otus.html
Step 13.2.2.	Qiime	Create a mapping file	http://qiime.org/documentation/file_formats.html.
Step 13.2.2.	Qiime	Validate a mapping file	http://qiime.org/scripts/validate_mapping_file.html.
Step 13.3.3.	Qiime	Link the OTU to sample description to mapping file	http://qiime.org/scripts/make_otu_network.html.
Step 13.3.4.	Qiime	Summarize Taxa through plots	http://qiime.org/scripts/summarize_taxa_through_plots.html.
Step 13.3.5.	Qiime	Biome Summarize table	http://biom-format.org/documentation/summarizing_biom_tables.html  In this study, all samples were rarified to 20,000 OTUs followed by analysis using alpha rarefaction script in QIIME.