We sincerely thank Dr. Mustafa Khokha, Yale University, for providing the use of his laboratory resources. We are grateful to Mr. Ming-Jie Wu for excellent technical assistance. EF is an HHMI investigator.This work was supported by a gift from the John Monsky and Jennifer Weis Monsky Lyme Disease Research Fund.

1. Preparation of DNA Templates
<ol>
	<li>Download the 16S rRNA sequence specific to each bacterial genera from the NCBI database and design polymerase chain reaction (PCR) compatible forward and reverse primers that will amplify genera-specific regions (~200 - 250 base-pair long) as described earlier19. Also refer to the open source databases SILVA20,21 and probeBase22 online resources for rRNA-targeted oligonucleotide probes and primers, as RNA probes for some bacterial genera may be commercially available. 
	Note: It is important to select gene regions that are specific to specific genera and ensure that designed primers do not amplify related bacterial genera. This is critical to obtain gene/genera-specific probe hybridization.</li>
	<li>Feed ticks for 24, 48 or 72 h on mice, dissect tick guts and prepare RNA and cDNA from tick guts as described earlier23. Use cDNA as template to PCR amplify genera-specific amplicons using a thermocycler. Run an aliquot of the PCR-product/amplicon on a 1.5% agarose gel and confirm that the amplicon corresponds to the expected size by visualization under ultraviolet (UV) light using a gel imaging system.</li>
	<li>Clone the bacterial 16S ribosomal RNA amplicon of interest into a commercially available TA vector (Table of Materials) containing RNA polymerase promoters suitable for bacteriophage polymerases (SP6, T7 or T3). Sequence the clones to confirm the identity of the amplicon and the directionality of the clone with respect to each of the promoters. Based on this, determine the promoter of choice to generate sense or antisense RNA probes (Figure 1).</li>
	<li>Linearize 1 mg of the plasmid with an appropriate restriction enzyme in a reaction volume of up to 30 &#181;Lfor 2 h at temperatures recommended by the manufacturer. Choose restriction enzymes based on the promoter that will be utilized to generate the sense or antisense probe (Figure 1). Verify linearization by visualization of 2 &#181;L of digest reaction on a 1% agarose gel.</li>
	<li>Purify the remaining 28 &#181;L of digested DNA using a commercially available PCR product column purification kit and quantify DNA concentration by spectrophotometer. 
	Note: Some sense probes may cause background staining much higher than the corresponding antisense probe and other options may need to be explored. Alternative negative controls include plasmids encoding sequences not represented in the sample or another probe that yields a distinctive pattern of hybridization.</li>
</ol>
2. Construction of Digoxygenin-UTP RNA Probes
<ol>
	<li>Prepare the nucleotide mix by combining 7.5 &#181;L of 100 mM UTP, 25 &#181;L of 10 mM digoxygenin-UTP, and 10 &#181;L each of 100 mM ATP, GTP, and CTP in a 1.5 mL centrifuge tube.</li>
	<li>Perform in vitro transcription using commercially available T7 or Sp6 RNA polymerase kits, using 1 &#181;L of the nucleotide mix (Step 2.1) and 0.25 - 1 &#181;g of template DNA. Bring the volume up to 20 &#181;L with water. Flick the tube to combine and pulse spin. Incubate at 37 &#176;C for 2.5 - 3 h. 
	Note: Probe construction has been successful with digested plasmid concentrations as low as 7 ng/&#181;L, but typical concentrations at this step range from 15 - 25 ng/&#181;L. The transcription reaction may also be incubated overnight at 37 &#176;C, but this does not significantly increase the RNA yield.</li>
	<li>Add 1 &#181;L of DNase (2,000 units/&#181;L) and incubate at 37 &#176;C for 10 min. Do not exceed 10 min, or the enzyme may begin degrading RNA.</li>
	<li>Add 30 &#181;L of ice-cold 7.5 - 8 M lithium chloride and 30 &#181;L of chilled nuclease-free water to precipitate the RNA. Flick the tube to mix. Allow precipitation of RNA to proceed overnight at -20 &#176;C.</li>
	<li>Collect RNA by centrifugation at 17,000 x g for 20 min at 4 &#176;C. Wash the pellet once with 1 mL of freshly prepared 75% ethanol in Diethyl pyrocarbonate (DEPC) water, then repeat centrifugation.</li>
	<li>Remove and discard the supernatant, invert the tube on a clean paper towel, and allow to dry for 10 min. Resuspend the pellet in nuclease-free water. If the pellet is easily visible, resuspend in 25 &#181;L. If the pellet is very small or not visible, resuspend in 15 - 20 &#181;L. Obtain an estimate of RNA concentration by spectrophotometer. 
	Note: Typical RNA concentrations range from 200 - 500 ng/&#181;L.</li>
</ol>
3. Visualization of RNA Probes by RNA Formaldehyde Gel Electrophoresis to Assess RNA Purity
CAUTION: Formaldehyde poses an inhalation hazard; therefore, generate the solutions required for RNA gel analysis in a fume hood. Ethidium bromide is a suspected carcinogen; handle with care.
<ol>
	<li>Prepare a 1% formaldehyde agarose gel as previously described24 and cast the gel in a gel box free of RNases. Once cool, fill the gel box with 1x running buffer (1x MOPS at pH 7.0, 5% formaldehyde).</li>
	<li>Prepare the Sample Buffer (5 &#181;L 400 mg/mL ethidium bromide, 20 &#181;L 10x MOPS, 35 &#181;L formaldehyde, and 100 &#181;L formamide). Combine 2 &#181;L of RNA probe (Step 2.6) with 8 &#181;L of Sample Buffer. Incubate at 70 &#176;C for 10 min.</li>
	<li>Prepare RNA Loading Buffer by combining 5 mL 50% glycerol, 1 mL 10% formaldehyde, 40 mg bromophenol blue, 40 mg xylene cyanol, and 20 &#181;L of 0.5 M EDTA (pH 7.5). After use, store this buffer at -20 &#176;C.</li>
	<li>Add 3 &#181;L of Loading Buffer to the RNA sample from Step 3.2 and mix. Keep sample tubes on ice.</li>
	<li>Load the entire sample volume from Step 3.4 into the gel. Load an aliquot of single-stranded RNA ladder alongside to verify RNA size. Run the gel at 100 V or lower until the blue dye migrates approximately 75% of the way down the gel. Visualize the RNA under UV light using a gel imaging system. &#160; 
	Note: &#160;A good quality RNA probe should appear as a discrete band with a mobility corresponding to the expected size of the probe (Figure 2, lane 1). If the probe appears as a diffuse and smeary band (Figure 2, lane 2) this should not be used.</li>
</ol>
4. Tick Gut Collection and Fixation
<ol>
	<li>Collect Ixodes scapularis nymphs that have fed on mice for the time points of interest. 
	Note: For the purposes of this technique, ticks fed for 48 or 72 h work best.&#160;</li>
	<li>Dissect the gut from the tick into MEMFA (Table 1) on a glass slide under a dissection microscope, avoiding damage to the organ as much as possible. Place a tick on a clean microscope slide in 20 - 30 &#181;L of MEMFA. Using a pair of sterile high-carbon steel razor blade #11 slice the head region at the scutum of the tick leaving the body of the tick. Gently press the body to push the gut diverticula and salivary glands out the body cuticle. Separate the salivary glands and the gut and scoop the guts on the razor blade.&#160;</li>
	<li>Collect guts into a 1.5 mL tube containing 500 &#181;L MEMFA. Incubate the tube at room temperature with gentle rocking for 1 h or overnight at 4 &#176;C. 
	Note: Tick salivary glands may also be dissected and similarly fixed and stained.</li>
	<li>Dehydrate the tissue by washing gently 3 times with 1 mL ice-cold 100% ethanol. Let the guts sink naturally to the bottom of the tube between each wash, as centrifugation may damage the tissue. For long-term storage, keep the samples in 100% ethanol at -20 &#176;C.</li>
</ol>
5. Construction of Mesh Sample Baskets and 24-well Basket Holder
<ol>
	<li>Cut the bottoms off of 2 mL or 5 mL snap-top centrifuge tubes using a heated single-edged razor blade on a scalpel. 
	CAUTION: The blade may need to be reheated several times before the cut is completed.</li>
	<li>Cut squares of a 110 &#181;m nylon mesh slightly larger than the new tube opening. Bond the mesh to the bottom of the tube by pressing them together lightly onto a hot plate on medium-low heat until a good seal is made. Let cool, ensure there are no gaps between the mesh and the tube, and trim excess mesh around the edges.&#160;</li>
	<li>Cut holes in the cover of a 24-well plate such that the lip of the sample basket made in Step 5.2 will sit at the hole and not fall through, yielding a set-up where the bottoms of the sample baskets will sit all the way in the wells when they are placed in the holes in the cover.</li>
	<li>Use this fitted basket holder to transfer baskets from one plate to another with relative ease for the entirety of the in situ hybridization protocol. Use two 24-well plates so that while one incubation is occurring, the other plate is prepared for the next wash.</li>
</ol>
6. In Situ Hybridization: Day 1 (Timing: 4 - 5 h)
<ol>
	<li>Transfer guts to labeled sample baskets, separated by experimental condition and intended RNA probe. 
	Note: Stain at least 5 guts per condition to account for natural variation among replicates.</li>
	<li>Rehydrate the samples gently to avoid introducing air bubbles into the tissue by gradually increasing the ratio of phosphate-buffered saline with 0.1 % non-ionic surfactant (PTw; Table 1) to ethanol in the washes. 
	Note: Complete all washes in the 24-well basket holder at ambient temperature with gentle agitation unless otherwise noted. Aliquot 500 - 600 &#181;L of wash solutions into each well of the holder such that the guts in each basket are completely submerged. Prepare all solutions with DEPC-treated water to prevent RNA degradation.
	<ol>
		<li>Wash the samples for 5 min in 500 &#181;L 100% ethanol.</li>
		<li>Prepare at least 500 &#181;L per sample basket of 75%, 50%, and 25% ethanol in PTw. Rehydrate the samples by washing for 5 min in each ethanol solution, moving from the highest ethanol concentration to the lowest.</li>
		<li>Wash the samples 4 times for 5 min each in PTw.</li>
	</ol>
	</li>
	<li>Permeabilize the samples with Proteinase K (10 &#181;g/mL) in PTw for 5 min.</li>
	<li>Prepare the tissue for hybridization with the RNA probes.
	<ol>
		<li>Wash the samples twice as described in 6.2 in the 24-well basket holder at ambient temperature with gentle agitation for 5 min each in 500 &#181;L triethanolamine buffer (0.1 M, pH 7.0 - 8.0) (Table 1) to maintain the samples in an amine-free environment.</li>
		<li>Treat the samples twice with 500 &#181;L 0.25% acetic anhydride in triethanolamine buffer (0.1 M, pH 7.0 - 8.0) for 5 min each, then wash the samples twice in PTw for 5 min each. 
		Note: The acetic anhydride acetylates free amines to neutralize positive charge, which is critical to prevent non-specific electrostatic interactions and ensure specific binding of the probe to mRNA.</li>
		<li>Fix the guts for 20 min with 500 &#181;L 4% paraformaldehyde in PTw, then wash 5 times in PTw for 5 min each.</li>
		<li>Prehybridize by incubating the samples in 500 &#181;L hybridization buffer /in the 24-well basket holder in the 24 well plate (Table 1) for 1.5 - 2.5 h at 60 &#176;C with gentle agitation in a shaking water bath. Save the hybridization buffer used for the prehybridization step to reuse in the Day 2 protocol (Step 7.1).</li>
		<li>Prepare probe hybridization solutions by diluting RNA probes in hybridization buffer to a final concentration of 1 &#181;g/mL. &#160;Incubate samples with probe hybridization solutions in the 24-well basket holder at 60 &#176;C with gentle agitation overnight in a shaking water bath (Table 2). Cover the plate carrying the basket holder snugly with aluminum foil to prevent evaporation of the hybridization solution.</li>
	</ol>
	</li>
</ol>
7. In Situ Hybridization: Day 2 (Timing: 4.5 - 5.5 h)
<ol>
	<li>Remove the samples from the probe hybridization solutions and place them into the reserved hybridization buffer from the previous day. Incubate at 60 &#176;C with gentle agitation for 3 min. 
	Note: Probe hybridization solutions may be stored at -20 &#176;C for reuse up to 3 times.</li>
	<li>Prepare 2x saline-sodium citrate buffer (SSC) by diluting 20x SSC in DEPC-treated water (Table 1). Wash the samples twice for 3 min with 2x SSC, then 3 times for 20 min with 2x SSC at 60 &#176;C to remove all traces of probe and hybridization buffer.</li>
	<li>Treat with RNase A (20 &#181;g/mL) and RNase T1 (10 &#181;g/mL) in 2x SSC for 30 min at 37 &#176;C to remove single stranded RNA probe representing free non-hybridized RNA.</li>
	<li>Wash once with 2x SSC for 10 min at room temperature. Prepare 0.2x SSC by diluting 2x SSC in DEPC-treated water, then wash twice with 0.2x&#160;SSC for 30 min at 60 &#176;C to remove excess RNases.</li>
	<li>Wash twice with 500 &#181;L of maleic acid buffer (MAB; Table 1) for 10 min each.</li>
	<li>Incubate samples with blocking solution (2% blocking reagent in MAB) for 1.5 - 2 h. 
	Note: The blocking reagent can be difficult to dissolve; gentle heating aids dissolution.</li>
	<li>Replace the blocking solution with anti-digoxigenin alkaline phosphatase-conjugated 500 &#181;L of antibody at a 1:3,000 dilution in blocking solution and incubate at room temperature for about 4 h or at 4 &#176;C overnight.</li>
</ol>
8. In Situ Hybridization: Day 3 (Timing: 6 h to overnight)
<ol>
	<li>Wash the samples at least 5 times for 30 min each with 500 &#181;L MAB to remove excess antibody. 
	Note: These washes are flexible and may be extended to 1 - 2 h, or 3 - 4 washes may be substituted for one overnight wash at 4 &#176;C with minimal effect on efficacy.</li>
	<li>Wash twice for 5 min with alkaline phosphatase buffer, pH 9.5 (AP buffer; Table 1).</li>
	<li>Begin the color reaction by replacing the last wash with 500 &#181;L of the chromogenic substrate for alkaline phosphatase (Table of Materials). Cover the sample plate with aluminum foil and let the staining proceed at room temperature for 3-&#160; 5 h or overnight at 4 &#176;C. Monitor the staining reaction periodically by viewing the tissue under a dissecting microscope to avoid overstaining. 
	Note: When the staining is complete, a purple tint is detectable by eye in the antisense-probed samples under the microscope, but the tissue should not be allowed to become very dark. Staining proceeds very slowly at 4 &#176;C and may take up to 20 - 24 h.</li>
	<li>Stop the color reaction by washing for 5 min in 500 &#181;L MAB, then fix the tissue overnight in Bouin&#8217;s solution. 
	CAUTION: Handle the Bouin&#8217;s solution in a fume hood; it is a corrosive carcinogen.</li>
</ol>
9. In Situ Hybridization: Day 4 (Timing: 3 - 3.5 h)
<ol>
	<li>Prepare at least 7 mL per sample basket of 1x SSC by diluting 20x SSC in DEPC-treated water. Remove the Bouin&#8217;s solution by washing the samples 4 to 6 times with 70% ethanol in 1x SSC until the tissue is no longer yellow.</li>
	<li>Prepare 500 &#181;L per sample basket of 75%, 50%, and 25% ethanol solutions in 1x SSC. Wash the samples for 5 min in each solution, moving from highest ethanol concentration to lowest to rehydrate the tissue. Wash twice for 5 min each in 1x SSC.</li>
	<li>Incubate the samples in the bleach solution (Table 1) for 90 min on a lightbox in a fume hood. 
	Note: This step allows any pigmentation in the samples or coloration from Bouins solution to be removed and enhances the probe signal for clear visualization.</li>
	<li>Wash the samples twice with 500 &#181;L of 1x SSC for 5 min.</li>
	<li>Relocate the guts with minimal damage by inverting the sample basket into a well of a new 24-well plate and wash with 70% ethanol through the mesh bottom using a transfer pipette. Store at -20 &#176;C if needed.</li>
	<li>To obtain an overview of the staining patterns of multiple samples as shown in Figure 3, maintain the guts in 70% ethanol in the 24 well-plate and view with any bright-field microscope. To examine individual guts under a bright-field microscope as shown in Figure 4, Figure 5, and Figure 6, mount the guts in 100% glycerol under coverslips. Use a plastic spatula to gently manipulate the tissue with minimal damage. 
	Note: The high viscosity of glycerol helps protect the tissue from damage by compression and allows the careful positioning of diverticula such that the tissue can be viewed optimally at higher magnifications.</li>
	<li>Capture images on the microscope using microscope specific image capture software (Table of Materials) and export as Tiff images to a generic image editing software. To quantify the relative staining differences between experimental treatments, download a generic image analysis software (Table of Materials). Open the image within the analysis software and use the instructions within the software to measure pixel intensity of the staining and compute histogram plots of the staining.</li>
</ol>

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K., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Techniques+and+probes+for+the+study+of+Xenopus+tropicalis+development.">Techniques and probes for the study of Xenopus tropicalis development.</a> Developmental Dynamics. 225 (4), 499-510 (2002).</li><li>Jowett, T., Lettice, L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Whole-mount+in+situ+hybridizations+on+zebrafish+embryos+using+a+mixture+of+digoxigenin-+and+fluorescein-labelled+probes.">Whole-mount in situ hybridizations on zebrafish embryos using a mixture of digoxigenin- and fluorescein-labelled probes.</a> Trends in Genetics. 10 (3), 73-74 (1994).</li><li>Behnam, F., Vilcinskas, A., Wagner, M., Stoecker, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+straightforward+DOPE+(double+labeling+of+oligonucleotide+probes)-FISH+(fluorescence+in+situ+hybridization)+method+for+simultaneous+multicolor+detection+of+six+microbial+populations.">A straightforward DOPE (double labeling of oligonucleotide probes)-FISH (fluorescence in situ hybridization) method for simultaneous multicolor detection of six microbial populations.</a> Applied Environmental Microbiology. 78 (15), 5138-5142 (2012).</li><li>Pai, V. P., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=HCN4+ion+channel+function+is+required+for+early+events+that+regulate+anatomical+left-right+patterning+in+a+nodal+and+lefty+asymmetric+gene+expression-independent+manner.">HCN4 ion channel function is required for early events that regulate anatomical left-right patterning in a nodal and lefty asymmetric gene expression-independent manner.</a> Biology Open. 6 (10), 1445-1457 (2017).</li><li>Legendre, F., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Whole+mount+RNA+fluorescent+in+situ+hybridization+of+Drosophila+embryos.">Whole mount RNA fluorescent in situ hybridization of Drosophila embryos.</a> JoVE. (71), e50057 (2013).</li></ol>

The authors have no conflicts of interest to disclose.

This is the first use of a whole-mount in situ hybridization (WMISH) technique to study the microbiota of an arthropod vector of pathogens. Our protocol was adapted from one used to study development in Drosophila and in frog embryos25,26. Whole-mount RNA in situ hybridization has been routinely used to localize gene transcripts spatially and temporally27 and visualization of transcripts can be done by bright-fie...

Human and livestock pathogens transmitted by arthropod vectors are found worldwide and account for about 20% of infectious diseases globally1, but effective and safe vaccines against most of these pathogens are not available. Our understanding of the important role of commensal, symbiotic and pathogenic microorganisms, collectively known as the microbiome2, in modulating and shaping the health of almost all metazoans3 is expanding. It is now evident that arthropod vectors of pathogens also harbor gut microbiota and these vector-associated microbiota have been shown to influence diverse vector-borne pathogens4,5. The arthropod microbiome is composed of eubacteria, archaea, viruses, and eukaryotic microbes such as protozoa, nematodes, and fungi6. However, the predominant research focus has been on eubacteria due, in part, to the availability of marker genes and reference databases to identify specific bacterial members.
With a focus on Ixodes scapularis, the tick vector of multiple human pathogens including Borrelia burgdorferi7, the causative agent of Lyme disease, the optimization of a microbial visualization technique was aimed at improving our understanding of tick gut microbiota in the context of vector-pathogen interactions. Several questions remain to be answered in the tick microbiome field. The gut is the site of the first extended encounter between the tick and the incoming pathogen in the context of horizontally transferred pathogens; therefore, understanding the role of vector gut microbiota in modulating vector-pathogen interactions will reveal meaningful insights. Ticks have a unique mode of blood meal digestion, where processing of blood meal components takes place intracellularly8. The gut lumen seemingly serves as a vessel to contain the blood meal as the tick feeds, and nutrient digestion and assimilation ensue throughout the several days of feeding and continue post-repletion. The pathogens acquired by the tick during feeding enter the gut lumen along with the bloodmeal and thus the lumen becomes a primary site of interactions among the tick, pathogen, and resident microbiota. As digestion proceeds through the repletion and Ixodid tick molting, the gut undergoes structural and functional changes9. The composition and the spatial organization of gut bacteria is also likely to vary in concert with the changing gut milieu. It is, therefore, important to understand the architecture of resident bacteria in the tick gut to fully understand the interplay of tick, pathogen, and gut microbiota.
Molecular techniques to describe host-associated microbiota routinely utilize high-throughput parallel sequencing strategies10 to amplify and sequence bacterial 16S ribosomal DNA (rDNA). These sequencing strategies circumvent the need to obtain axenic cultures of specific bacteria and provide an in-depth description of all bacterial members represented in the sample. Nevertheless, such strategies are confounded by the inability to distinguish environmental contaminations from bona fide residents. Further, when assessing samples, such as ticks, that are small in size and hence contain low microbiota-specific DNA yields, the likelihood of amplification of environmental contaminants is increased11 and results in the ambiguous interpretation of microbiome composition. Functional characterization in conjunction with the visualization of specific viable bacteria will, therefore, be critical to define and discern the microbiome of the tick temporally and spatially. Towards this goal, we took advantage of the whole-mount RNA in situ hybridization. This technique is routinely used to assess gene expression patterns in organs and embryos12,13,14 and allows semiquantitative analysis of expression over the entire sample of interest. This differs from traditional in situ hybridization techniques which utilize tissue sections and often require extensive analysis of sectioned material with a computational assembly to predict expression in whole organs15. While whole-mount generally refers to whole organisms12, here whole-mount refers to whole guts or organs. The advantages of using the whole-mount RNA in situ hybridization approach to assess the architecture of tick gut microbiota are multifold. The tick gut is composed of 7 pairs of diverticula, each pair varying in size16. The functional differences, if any, among these diverticula, are not understood in the context of tick biology, tick microbiota or tick-pathogen interactions. Manipulations of the gut that rupture the gut diverticula would displace microbiota present in the gut lumen or those associated loosely with the gut and result in misinterpretation of the spatial localization of microbiota. Fluorescence-labeled RNA in situ hybridization has been utilized earlier to examine tick gut transcripts17 by fixing and opening individual gut diverticula to ensure probe hybridization and to localize B. burgdorferi transcripts by sectioning paraffin-embedded whole ticks18. Both these approaches require manipulations of the tick tissues prior to hybridization that would affect the gut microbiota architecture.
In this report, we describe in detail the protocol to examine viable tick gut microbiota using whole-mount in situ hybridization (WMISH). The use of whole-mount RNA in situ hybridization enables a global understanding of the presence and abundance of specific gut bacteria in the different regions of the gut and may spur new insights into tick gut biology in the context of pathogen colonization and transmission. Further, the use of RNA probes directed against specific bacterial RNA allows detection of viable bacteria in the tick gut.

<table><tbody><tr><td>Sefar NITEX Nylon Mesh, 110 micron</td><td>Amazon</td><td>03-110/47</td><td></td></tr><tr><td>pGEM-T Easy Vector System</td><td>Promega</td><td>A1360</td><td></td></tr><tr><td>Digoxygenin-11-UTP</td><td>Roche</td><td>1209256910</td><td></td></tr><tr><td>dNTP</td><td>New England Biolabs&amp;nbsp;</td><td>N0447S</td><td></td></tr><tr><td>DNAse I(RNAse-free)</td><td>New England Biolabs</td><td>M0303S</td><td></td></tr><tr><td>HiScribe SP6 RNA synthesis kit</td><td>New England Biolabs</td><td>E2070S</td><td></td></tr><tr><td>HiScribe T7 High Yield RNA Synthesis Kit</td><td>New England Biolabs</td><td>E2040S</td><td></td></tr><tr><td>Water, RNase-free, DEPC-treated</td><td>American Bioanalytical</td><td>AB02128-00500</td><td></td></tr><tr><td>EDTA, 0.5M, pH 8.0</td><td>American Bioanalytical</td><td>AB00502-01000</td><td></td></tr><tr><td>Formaldehyde, 37%</td><td>JT Baker</td><td>2106-01</td><td></td></tr><tr><td>Formamide</td><td>American Bioanalytical</td><td>AB00600-00500</td><td></td></tr><tr><td>EGTA</td><td>Sigma Aldrich</td><td>E-4378</td><td></td></tr><tr><td>DPBS, 10X</td><td>Gibco</td><td>14300-075</td><td></td></tr><tr><td>Tween-20</td><td>Sigma Aldrich</td><td>P1379-25ML</td><td></td></tr><tr><td>Proteinase K</td><td>Sigma Aldrich</td><td>3115879001</td><td></td></tr><tr><td>Triethanolamine HCl</td><td>Sigma Aldrich</td><td>T1502-100G</td><td></td></tr><tr><td>Acetic anhydride</td><td>Sigma Aldrich</td><td>320102-100ML</td><td></td></tr><tr><td>Paraformaldehyde</td><td>ThermoScientific/Pierce</td><td>28906</td><td></td></tr><tr><td>SSC, 20X</td><td>American Bioanalytical</td><td>AB13156-01000</td><td></td></tr><tr><td>RNA from torula yeast</td><td>Sigma Aldrich</td><td>R3629-5G</td><td></td></tr><tr><td>Heparin, sodium salt</td><td>Sigma Aldrich</td><td>H3393-10KU</td><td></td></tr><tr><td>Denhardt&#039;s Solution, 50X</td><td>Sigma Aldrich</td><td>D2532-5ML</td><td></td></tr><tr><td>CHAPS hydrate</td><td>Sigma Aldrich</td><td>C3023-1G</td><td></td></tr><tr><td>RNase A</td><td>Sigma Aldrich</td><td>10109142001</td><td></td></tr><tr><td>RNase T1</td><td>ThermoScientific&amp;nbsp;</td><td>EN0541</td><td></td></tr><tr><td>Maleic acid</td><td>Sigma Aldrich</td><td>M0375-100G</td><td></td></tr><tr><td>Blocking reagent</td><td>Sigma Aldrich</td><td>11096176001</td><td></td></tr><tr><td>Anti-Digoxigenin-AP, Fab fragments</td><td>Sigma Aldrich</td><td>11093274910</td><td></td></tr><tr><td>Levamisol hydrochloride</td><td>Sigma Aldrich</td><td>31742-250MG</td><td></td></tr><tr><td>Chromogenic substrate for alkaline phosphatase</td><td>Sigma Aldrich</td><td>11442074001</td><td></td></tr><tr><td>Bouin&#039;s solution</td><td>Sigma Aldrich</td><td>HT10132-1L</td><td></td></tr><tr><td>Hydrogen peroxide</td><td>Mallinkrodt Baker, Inc</td><td>2186-01</td><td></td></tr><tr><td>Single stranded RNA ladder</td><td>Ambion -Millenium</td><td>AM7151</td><td></td></tr><tr><td>&amp;nbsp;#11 High-Carbon steel blades&amp;nbsp;</td><td>C and A Scientific Premiere</td><td>#11-9411</td><td></td></tr><tr><td>Thermocycler</td><td>BioRad, CA</td><td>1851148</td><td></td></tr><tr><td>Spectrophotometer</td><td>ThermoScientific&amp;nbsp;</td><td>NanoDrop 2000C</td><td></td></tr><tr><td>Orbital shaker</td><td>VWR</td><td>DS-500E Digital Orbital shaker</td><td></td></tr><tr><td>Shaking water bath</td><td>BELLCO Glass, Inc</td><td>Hot Shaker-7746-12110</td><td></td></tr><tr><td>Gel&amp;nbsp; documentation system</td><td>BioRad</td><td>Gel Doc XR+ Gel documentation system</td><td></td></tr><tr><td>Bright-field Microscope&amp;nbsp;</td><td>Nikon</td><td>NikonSM2745T</td><td></td></tr><tr><td>Bright-field Microscope&amp;nbsp;</td><td>Zeiss</td><td>AXIO Scope.A1</td><td></td></tr><tr><td>Dissection microscope&amp;nbsp;</td><td>Zeiss</td><td>STEMI 2000-C</td><td></td></tr><tr><td>&amp;nbsp;Light box</td><td>VWR</td><td>102097-658</td><td></td></tr><tr><td>PCR purification kit&amp;nbsp;</td><td>Qiagen</td><td>28104</td><td></td></tr><tr><td>Image capture software</td><td>Zeiss</td><td>Zen lite</td><td></td></tr><tr><td>Image editing software&amp;nbsp;</td><td>Adobe&amp;nbsp;</td><td>Adobe Photoshop CS4 version 11.0</td><td></td></tr><tr><td>Image analysis software</td><td>National Institutes of Health</td><td>ImageJ-NIH /imagej.nih.gov/ij/</td><td></td></tr><tr><td>Automation compatible instrumentation</td><td>Intavis Bioanalytical Instruments, Tubingen, Germany).&amp;nbsp;</td><td>Intavis, Biolane HT1.16v</td><td></td></tr></tbody></table>

visualization of microbiota in tick guts by whole-mount in situ hybridization

Infectious diseases transmitted by arthropod vectors continue to pose a significant threat to human health worldwide. The pathogens causing these diseases, do not exist in isolation when they colonize the vector; rather, they likely engage in interactions with resident microorganisms in the gut lumen. The vector microbiota has been demonstrated to play an important role in pathogen transmission for several vector-borne diseases. Whether resident bacteria in the gut of the Ixodes scapularis tick, the vector of several human pathogens including Borrelia burgdorferi, influence tick transmission of pathogens is not determined. We require methods for characterizing the composition of the bacteria associated with the tick gut to facilitate a better understanding of potential interspecies interactions in the tick gut. Using whole-mount in situ hybridization to visualize RNA transcripts associated with particular bacterial species allows for the collection of qualitative data regarding the abundance and distribution of the microbiota in intact tissue. This technique can be used to examine changes in the gut microbiota milieu over the course of tick feeding and can also be applied to analyze expression of tick genes. Staining of whole tick guts yield information about the gross spatial distribution of target RNA in the tissue without the need for three-dimensional reconstruction and is less affected by environmental contamination, which often confounds the sequencing-based methods frequently used to study complex microbial communities. Overall, this technique is a valuable tool that can be used to better understand vector-pathogen-microbiota interactions and their role in disease transmission.

The measurement and estimation of the quality of the RNA probes are critical prior to beginning the staining. In vitro transcription efficiency depends highly on the amount and quality of the DNA template. We routinely visualized the RNA probes on a formaldehyde gel to verify the purity and amount of probe generated by the transcription reactions. The probes should appear as bright, discrete bands (Figure 2). Spectrophotometric measurements of RNA co...

Watch this Scientific Journal Video about Visualization of Microbiota in Tick Guts by Whole-mount In Situ Hybridization at JoVE.com

Visualization of Microbiota in Tick Guts by Whole-mount In Situ Hybridization

Here, we present a protocol to spatially and temporally assess the presence of viable microbiota in tick guts using a modified whole-mount in situ hybridization approach.

Visualization of Microbiota in Tick Guts by Whole-mount In Situ Hybridization

Infectious diseases transmitted by arthropod vectors continue to pose a significant threat to human health worldwide. The pathogens causing these ...

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Research

JoVE Journal

Genetics

9.5K Views.  Yale University School of Medicine. Here, we present a protocol to spatially and temporally assess the presence of viable microbiota in tick guts using a modified whole-mount in situ hybridization approach.

Video: Visualization of Microbiota in Tick Guts by Whole-mount In Situ Hybridization

In Situ Labeling of Mitochondrial DNA Replication in Drosophila Adult Ovaries by EdU Staining

The mitochondrial genome is inherited exclusively through the maternal line. Understanding of how the mitochondrion and its genome are proliferated and transmitted from one generation to the next through the female oocyte is of fundamental importance. Because of the genetic tractability, and the elegant, ordered simplicity by which oocyte development proceeds, Drosophila oogenesis has become an invaluable system for mitochondrial study. An EdU (5-ethynyl-2&#180;-deoxyuridine) labeling method was utilized to detect mitochondrial DNA (mtDNA) replication in Drosophila ovaries. This method is superior to the BrdU (5-bromo-2'-deoxyuridine) labeling method in that it allows for good structural preservation and efficient fluorescent dye penetration of whole-mount tissues.
Here we describe a detailed protocol for labeling replicating mitochondrial DNA in Drosophila adult ovaries with EdU. Some technical solutions are offered to improve the viability of the ovaries, maintain their health during preparation, and ensure high-quality imaging. Visualization of newly synthesized mtDNA in the ovaries not only reveals the striking temporal and spatial pattern of mtDNA replication through oogenesis, but also allows for simple quantification of mtDNA replication under various genetic and pharmacological perturbations.

In Situ Labeling of Mitochondrial DNA Replication in Drosophila Adult Ovaries by EdU Staining

Drosophila oogenesis continues to be exceptionally useful in the study of mitochondrial proliferation and inheritance. This manuscript describes a detailed protocol used to label the replicating mitochondrial DNA (mtDNA) in Drosophila adult ovaries with 5-ethynyl-2&#180;-deoxyuridine (EdU), which facilitates uncovering mechanisms associated with mitochondrial inheritance that were previously debatable.

The mitochondrial genome is inherited exclusively through the maternal line. Understanding of how the mitochondrion and its genome are proliferated and ...

Optogenetic Random Mutagenesis Using Histone-miniSOG in C. elegans

Forward genetic screening in model organisms is the workhorse to discover functionally important genes and pathways in many biological processes. In most mutagenesis-based screens, researchers have relied on the use of toxic chemicals, carcinogens, or irradiation, which requires designated equipment, safety setup, and/or disposal of hazardous materials. We have developed a simple approach to induce heritable mutations in C. elegans using germline-expressed histone-miniSOG, a light-inducible potent generator of reactive oxygen species. This mutagenesis method is free of toxic chemicals and requires minimal laboratory safety and waste management. The induced DNA modifications include single-nucleotide changes and small deletions, and complement those caused by classical chemical mutagenesis. This methodology can also be used to induce integration of extrachromosomal transgenes. Here, we provide the details of the LED setup and protocols for standard mutagenesis and transgene integration.

Optogenetic Random Mutagenesis Using Histone-miniSOG in C. elegans

Genetically-encoded histone-miniSOG induces genome-wide heritable mutations in a blue&#160;light-dependent manner. This mutagenesis method is simple, fast, free of toxic chemicals, and well-suited for forward genetic screening and transgene integration.

Forward genetic screening in model organisms is the workhorse to discover functionally important genes and pathways in many biological processes. In most ...

Detection of Inter-chromosomal Stable Aberrations by Multiple Fluorescence In Situ Hybridization (mFISH) and Spectral Karyotyping (SKY) in Irradiated Mice

Ionizing radiation (IR) induces numerous stable and unstable chromosomal aberrations. Unstable aberrations, where chromosome morphology is substantially compromised, can easily be identified by conventional chromosome staining techniques. However, detection of stable aberrations, which involve exchange or translocation of genetic materials without considerable modification in the chromosome morphology, requires sophisticated chromosome painting techniques that rely on in situ hybridization of fluorescently labeled DNA probes, a chromosome painting technique popularly known as fluorescence in situ hybridization (FISH). FISH probes can be specific for whole chromosome/s or precise sub-region on chromosome/s. The method not only allows visualization of stable aberrations, but it can also allow detection of the chromosome/s or specific DNA sequence/s involved in a particular aberration formation. A variety of chromosome painting techniques are available in cytogenetics; here two highly sensitive methods, multiple fluorescence in situ hybridization (mFISH) and spectral karyotyping (SKY), are discussed to identify inter-chromosomal stable aberrations that form in the bone marrow cells of mice after exposure to total body irradiation. Although both techniques rely on fluorescent labeled DNA probes, the method of detection and the process of image acquisition of the fluorescent signals are different. These two techniques have been used in various research areas, such as radiation biology, cancer cytogenetics, retrospective radiation biodosimetry, clinical cytogenetics, evolutionary cytogenetics, and comparative cytogenetics.

Detection of Inter-chromosomal Stable Aberrations by Multiple Fluorescence In Situ Hybridization mFISH and Spectral Karyotyping SKY in Irradiated Mice

The present protocol describes the usefulness of multiple fluorescence in situ hybridization (mFISH) and spectral karyotyping (SKY) in identifying inter-chromosomal stable aberrations in the bone marrow cells of mice after exposure to total body irradiation.

Ionizing radiation (IR) induces numerous stable and unstable chromosomal aberrations. Unstable aberrations, where chromosome morphology is substantially ...

Methods for Rapid Transfer and Localization of Lyme Disease Pathogens Within the Tick Gut

Lyme disease is caused by infection with the spirochete pathogen Borrelia burgdorferi, which is maintained in nature by a tick-rodent infection cycle 1. A tick-borne murine model 2 has been developed to study Lyme disease in the laboratory. While na&iacute;ve ticks can be infected with B. burgdorferi by feeding them on infected mice, the molting process takes several weeks to months to complete. Therefore, development of more rapid and efficient tick infection techniques, such as a microinjection-based procedure, is an important tool for the study of Lyme disease 3,4. The procedure requires only hours to generate infected ticks and allows control over the delivery of equal quantities of spirochetes in a cohort of ticks. This is particularly important as the generation of B. burgdorferi infected ticks by the natural feeding process using mice fails to ensure 100% infection rate and potentially results in variation of pathogen burden amongst fed ticks. Furthermore, microinjection can be used to infect ticks with B. burgdorferi isolates in cases where an attenuated strain is unable to establish infection in mice and thus can not be naturally acquired by ticks 5. This technique can also be used to deliver a variety of other biological materials into ticks, for example, specific antibodies or double stranded RNA 6. In this article, we will demonstrate the microinjection of nymphal ticks with in vitro-grown B. burgdorferi. We will also describe a method for localization of Lyme disease pathogens in the tick gut using confocal immunofluorescence microscopy.

Lyme disease research studies often require generation of ticks infected with the pathogen Borrelia burgdorferi, a process that typically takes several weeks. Here we demonstrate a microinjection-based tick infection procedure that can be accomplished within hours. We also demonstrate an immunofluorescence method for in situ localization of B. burgdorferi within ticks.

Lyme disease is caused by infection with the spirochete pathogen Borrelia burgdorferi, which is maintained in nature by a tick-rodent infection cycle 1.  ...

Immunology and Infection

Feeding of Ticks on Animals for Transmission and Xenodiagnosis in Lyme Disease Research

Transmission of the etiologic agent of Lyme disease, Borrelia burgdorferi, occurs by the attachment and blood feeding of Ixodes species ticks on mammalian hosts. In nature, this zoonotic bacterial pathogen may use a variety of reservoir hosts, but the white-footed mouse (Peromyscus leucopus) is the primary reservoir for larval and nymphal ticks in North America. Humans are incidental hosts most frequently infected with B. burgdorferi by the bite of ticks in the nymphal stage. B. burgdorferi adapts to its hosts throughout the enzootic cycle, so the ability to explore the functions of these spirochetes and their effects on mammalian hosts requires the use of tick feeding. In addition, the technique of xenodiagnosis (using the natural vector for detection and recovery of an infectious agent) has been useful in studies of cryptic infection. In order to obtain nymphal ticks that harbor B. burgdorferi, ticks are fed live spirochetes in culture through capillary tubes. Two animal models, mice and nonhuman primates, are most commonly used for Lyme disease studies involving tick feeding. We demonstrate the methods by which these ticks can be fed upon, and recovered from animals for either infection or xenodiagnosis.

Lyme disease is the most commonly-reported vector-borne disease in North America. The causative agent, Borrelia burgdorferi is a spirochete bacterium transmitted by Ixodid ticks. Transmission and detection of infection in animal models is optimized by the use of tick feeding, which we describe here.

Transmission of the etiologic agent of Lyme disease, Borrelia burgdorferi, occurs by the  attachment and blood feeding of Ixodes species ticks on ...

Visualization of Candida albicans in the Murine Gastrointestinal Tract Using Fluorescent In Situ Hybridization

Candida albicans is a fungal component of the gut microbiota in humans and many other mammals. Although C. albicans does not cause symptoms in most colonized hosts, the commensal reservoir does serve as a repository for infectious disease, and the presence of high fungal titers in the gut is associated with inflammatory bowel disease. Here, we describe a method to visualize C. albicans cell morphology and localization in a mouse model of stable gastrointestinal colonization. Colonization is established using a single dose of C. albicans in animals that have been treated with oral antibiotics. Segments of gut tissue are fixed in a manner that preserves the architecture of luminal contents (microorganisms and mucus) as well as the host mucosa. Finally, fluorescent in situ hybridization is performed using probes against fungal rRNA to stain for C. albicans and hyphae. A key advantage of this protocol is that it allows for simultaneous observation of C. albicans cell morphology and its spatial association with host structures during gastrointestinal colonization.

Visualization of Candida albicans in the Murine Gastrointestinal Tract Using Fluorescent In Situ Hybridization

The purpose of this protocol is to visualize Candida albicans cell shape and localization in the mammalian gastrointestinal tract.

Candida albicans is a fungal component of the gut microbiota in humans and many other mammals. Although C. albicans does not cause symptoms in most ...

Visualization of Gut Microbiota-host Interactions via Fluorescence In Situ Hybridization, Lectin Staining, and Imaging

Measuring the localization of microbes within their in vivo context is an essential step in revealing the functional relationships between the microbiota and the vertebrate gut. The spatial landscape of the gut microbiota is tightly controlled by physical features - intestinal mucus, crypts, and folds - and is affected by host-controlled properties such as pH, oxygen availability, and immune factors. These properties limit the ability of commensal microbes and pathogens alike to colonize the gut stably. At the micron-scale, microbial organization determines the close-range interactions between different microbes as well as the interactions between microbes and their host. These interactions then affect large-scale organ function and host health.
This protocol enables the visualization of the gut microbiota spatial organization from distances between cells to organ-wide scales. The method is based on fixing gut tissues while preserving intestinal structure and mucus properties. The fixed samples are then embedded, sectioned, and stained to highlight specific bacterial species through fluorescence in situ hybridization (FISH). Host features, such as mucus and host cell components, are labeled with fluorescently labeled lectins. Finally, the stained sections are imaged using a confocal microscope utilizing tile-scan imaging at high magnification to bridge the micron to centimeter length scales. This type of imaging can be applied to intestinal sections from animal models and biopsies from human tissues to determine the biogeography of the microbiota in the gut in health and disease.

Visualization of Gut Microbiota-host Interactions via Fluorescence In Situ Hybridization, Lectin Staining, and Imaging

This streamlined protocol details a workflow to detect and image bacteria in complex tissue samples, from fixing the tissue to staining microbes with fluorescent in situ hybridization.

Measuring the localization of microbes within their in vivo context is an essential step in revealing the functional relationships between the microbiota ...

Whole&#45;Organ Pathogen Tracking via Fluorescent Reporter Quantification

High&#45;Resolution Three&#45;Dimensional Whole&#45;Organ Tomography of Microbial Infections

Most infections take place within three-dimensional host tissues with intricate anatomy and locally varying host physiology. The positioning of pathogen cells within this diverse environment significantly affects their stress levels, responses, fate, and contribution to the overall progression of the disease and treatment failure. However, due to the technical difficulties in locating &#181;m-sized pathogen cells within cm-sized host organs, this area of research has been relatively unexplored. Here, we present a method for addressing this challenge. We employ serial two-photon tomography and AI-enhanced image analysis to locate individual Salmonella cells throughout the entire spleen, liver lobes, and whole lymph nodes of infected mice. Using fluorescent reporters and in vivo antibody administration, the replication rate of single Salmonella cells, their local interaction with specific immune cells, and bacterial responses to antibiotics can be determined. These methodologies open avenues for a comprehensive examination of infections, their prevention, and treatment within the three-dimensional tissue context.

Author Spotlight: Unraveling Bacterial Responses to Antibiotics and Immune System in Tissues

Here, we describe a procedure that enables organ-wide detection of pathogenic bacteria during infection and quantification of fluorescent reporter activities.

Most infections take place within three-dimensional host tissues with intricate anatomy and locally varying host physiology. The positioning of pathogen ...

Tick Microbiome Characterization by Next-Generation 16S rRNA Amplicon Sequencing

In recent decades, vector-borne diseases have re-emerged and expanded at alarming rates, causing considerable morbidity and mortality worldwide. Effective and widely available vaccines are lacking for a majority of these diseases, necessitating the development of novel disease mitigation strategies. To this end, a promising avenue of disease control involves targeting the vector microbiome, the community of microbes inhabiting the vector. The vector microbiome plays a pivotal role in pathogen dynamics, and manipulations of the microbiome have led to reduced vector abundance or pathogen transmission for a handful of vector-borne diseases. However, translating these findings into disease control applications requires a thorough understanding of vector microbial ecology, historically limited by insufficient technology in this field. The advent of next-generation sequencing approaches has enabled rapid, highly parallel sequencing of diverse microbial communities. Targeting the highly-conserved 16S rRNA gene has facilitated characterizations of microbes present within vectors under varying ecological and experimental conditions. This technique involves amplification of the 16S rRNA gene, sample barcoding via PCR, loading samples onto a flow cell for sequencing, and bioinformatics approaches to match sequence data with phylogenetic information. Species or genus-level identification for a high number of replicates can typically be achieved through this approach, thus circumventing challenges of low detection, resolution, and output from traditional culturing, microscopy, or histological staining techniques. Therefore, this method is well-suited for characterizing vector microbes under diverse conditions but cannot currently provide information on microbial function, location within the vector, or response to antibiotic treatment. Overall, 16S next-generation sequencing is a powerful technique for better understanding the identity and role of vector microbes in disease dynamics.

Here we present a next-generation sequencing protocol for 16S rRNA sequencing which enables identification and characterization of microbial communities within vectors. This method involves DNA extraction, amplification and barcoding of samples through PCR, sequencing on a flow-cell, and bioinformatics to match sequence data to phylogenetic information.

In recent decades, vector-borne diseases have re-emerged and expanded at alarming rates, causing considerable morbidity and mortality worldwide. Effective ...

Biology

Visualization of Bacteria in Bladder Biopsy Sections via Fluorescence In Situ Hybridization

Prepare a humidifying chamber for each probe by adding a soaked, crumpled, delicate task wipe and sterile water to the reservoir of a P1000 tip box. Place the tip holder cartridge on top, as this is where the slides will sit. When the final wash is complete, remove the slide from the slide rack, and place them onto a fresh paper towel, tissue-side up. Use a delicate task wipe to dry the slide, being careful to only gently dab near but not on the biopsy section to wick away the water. Using a hydrophobic pen, draw a border around the biopsy section, and place the slide tissue-side up in the humidifying chamber.
Next, place the humidifying chamber into an incubator set to 50 degrees Celsius. Pipette between 50 and 150 microliters of the staining solution directly on top of the tissue so that the rectangle made by the hydrophobic border around the tissue is filled, and close the box gently. Incubate overnight at 50 degrees Celsius in the dark. If the incubator has a window, cover it with aluminum foil to create a dark environment.
The next morning, remove the slides from the humidifying chambers, and quickly wick away any remaining hybridization solution with a delicate task wipe. Then, place the slides into a vertical staining rack. Place the staining rack into an aluminum foil-wrapped coplin jar containing 100ml of the pre-warmed wash buffer for 10 minutes. Repeat this wash step two more times with fresh wash buffer in new coplin jars.
During these wash steps, prepare the counterstain by diluting a stock solution of Hoechst 33342 in wash buffer at a ratio of 1 to 1,000. To the same tube, add Alexa-555 wheat germ agglutinin to a final concentration of five micrograms per milliliter and Alexa-555 phalloidin to a final concentration of 33 nanomolar. Store in the dark until ready to use.
When the final wash is complete, remove the slides from the coplin jar, and gently wick away any excess wash buffer with a delicate task wipe. Place the slides tissue-side up on a paper towel, and add between 50 and 150 microliters of counterstain directly on top of the tissue so that the hydrophobic border is filled but not overflowing. Cover up to four slides with a cryobox top, and incubate at room temperature for 10 minutes.
After this, place the slides back into the staining rack, and wash them twice more in coplin jars containing fresh wash buffer, with each wash lasting 10 minutes. Then, thoroughly dry the slides, and place them tissue-side up on a paper towel under a cryobox top. Squeeze one drop of mounting media directly on top of the tissue, and gently place an appropriately-sized coverslip on top. Gently, press out any bubbles, and allow the cover-slipped slides to cure overnight in the dark. The next day, seal the edges of the coverslips to the slide with a light coat of clear nail polish, and let dry in the dark for 10 minutes, before storing them in the dark at 4 degrees Celsius.
When ready to image the stained biopsies, switch on the confocal microscope and the software associated with the microscope. Start with a FISH-positive slide and switch to the computer visualization mode. Select the channels for 405, 488, and 555. Set the pinhole using the longest wavelength channel, which in this case is 555. Then, find the current focal plane for visualization of labeled bacteria in the 488 channel. Without changing the focal plane, set the gain, laser power, and offset for each channel, such that the signal is not saturated, and the background is not overcorrected. Acquire the image in all three channels.

Visualization of Microbiota in Tick Guts by Whole-mount In Situ Hybridization

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