This research was supported by grants from the Natural Sciences and Engineering Research Council of Canada (Grant No. ALLRP 570780-2021) and McMaster University.

NOTE: Any steps utilizing international soil samples and/or A. fumigatus spores and mycelia require working within a biosafety cabinet for level 2 organisms (BSCII).
1. Isolation of yeast from soil
<ol>
	<li>Preparation of antibacterial and antifungal solutions
	<ol>
		<li>Suspend chloramphenicol powder in 70% ethanol to prepare a 50 g/L stock solution. Sterilize by syringe filtration and store at 4 &#176;C. 
		&#8203;NOTE: This antibiotic will prevent the growth of most bacteria during soil yeast isolation. As chloramphenicol-resistant bacteria may still grow, colony morphology must be carefully taken into consideration when distinguishing yeasts from bacteria. Additional antibiotics may be added to media when working with soil suspected of containing antibiotic-resistant bacterial strains. Bacterial contamination in chloramphenicol-supplemented media was not an issue encountered when isolating yeasts from environmental soils.</li>
		<li>Suspend benomyl powder in DMSO to prepare a 5 g/L stock solution. Sterilize by syringe filtration and store at 4 &#176;C. 
		NOTE: This selective antifungal drug prevents the growth of most filamentous fungi without affecting yeast growth during soil yeast isolation26,27.</li>
	</ol>
	</li>
	<li>Preparation of culture media and sterile equipment
	<ol>
		<li>To prepare YEPD (Yeast Extract-Peptone-Dextrose) broth, add 10 g of Yeast Extract, 20 g of peptone, and 20 g of dextrose to 1 L of double-distilled water. Stir until well-mixed and autoclave for 40 min at 121 &#176;C. Store at room temperature until use.</li>
		<li>YEPD solid agar medium
		<ol>
			<li>Mix 10 g of yeast extract, 20 g of peptone, 20 g of dextrose, and 20 g of agar in 1 L of water. Stir well to mix and autoclave for 40 min at 121 &#176;C.</li>
			<li>Once sufficiently cooled, add 1 mL of chloramphenicol and benomyl from stock solutions to bring the final concentrations of the two antimicrobials to 50 mg/L and 5 mg/L, respectively.</li>
			<li>Mix well by stirring and pour into 10 cm diameter Petri dishes. Leave at room temperature overnight to set and store at 4 &#176;C until use. 
			NOTE: From 1 L of YEPD, approximately 40 plates can be poured.</li>
		</ol>
		</li>
		<li>Sterilize wooden plain-tipped applicator sticks and reusable cell spreaders by autoclaving and store at room temperature.</li>
	</ol>
	</li>
	<li>Incubation of soil in liquid broth
	<ol>
		<li>Prepare a set of sterile 13 mL culture tubes by labeling them with soil sample ID.</li>
		<li>Using a serological pipette, add 5 mL of YEPD broth supplemented with chloramphenicol and benomyl into each tube.</li>
		<li>Working in a BSCII, transfer ~0.1 g of soil into the appropriate culture tube using a sterile, wooden plain-tipped applicator. 
		NOTE: Use a fresh applicator for each soil sample and discard immediately upon use to avoid cross-contamination between samples.</li>
		<li>Cap the tube securely to the first stop to prevent spillage but still allow air exchange during incubation. Incubate the culture tubes in a roller drum for 24 h at a temperature deemed optimum for maximizing yeast growth. 
		NOTE: The incubation temperature should be decided based on the mean annual temperature of the soil samples&#39; country of origin. For example, when isolating soil yeasts from Iceland, the culture tubes were incubated at 14 &#176;C, whereas soils from Saudi Arabia were incubated at 30 &#176;C. Due to slower yeast growth at lower temperatures, incubation time might have to be extended for up to 72 h.</li>
	</ol>
	</li>
	<li>Transfer the supernatant to the solid medium.
	<ol>
		<li>Using the set of YEPD + chloramphenicol + benomyl agar plates prepared in Step 1.2, label them with the soil sample ID.</li>
		<li>Remove the culture tubes prepared in Step 1.3 from the roller drum. Working in a BSCII, briefly vortex the tube to draw soil particles and cells that may have settled at the bottom back into suspension.</li>
		<li>Using a micropipette, transfer 100 &#181;L of the supernatant onto a plate. Use a sterile, reusable cell spreader to spread the liquid thoroughly and evenly over the agar surface. 
		NOTE: Working in sets of 10 samples can significantly speed up this process. Pipette the supernatant onto 10 plates first and then perform spreading. Use a fresh spreader for each sample to avoid cross-contamination between samples.</li>
		<li>Stack the plates in plastic bags, seal, and incubate upside down for 2-3 days at the same temperature used previously for liquid broth incubation until microbial growth is visible.</li>
	</ol>
	</li>
	<li>Detection of yeasts and streaking for single colonies
	<ol>
		<li>After allowing for sufficient incubation time (typically 2-3 days, but may take longer at lower temperatures), inspect the plates in a BSCII for any yeast growth. Look for creamy, round, matte-like yeasts that are easily distinguished from bacterial and mold colonies. 
		NOTE: Some yeasts produce colored pigments and may appear black/brown, yellow, or red, but their overall colony texture and shape would be similar to non-pigmented yeasts.</li>
		<li>Select one yeast-like colony from each plate for further processing. 
		NOTE: If more than one type of morphology is observed on a single plate, select one representative colony for each morphological type.</li>
		<li>Using sterile, wooden plain-tipped applicator sticks, transfer each selected colony onto a fresh YEPD + chloramphenicol + benomyl plate and streak for single colonies. Perform three separate streaks.
		<ol>
			<li>Streak back and forth over a third of the plate using an applicator stick. Begin the second and third streak by streaking the applicator across the preceding streak once. Use a new applicator stick for every streak. 
			NOTE: Use one plate per isolate. Discard applicators immediately upon use to avoid cross-contamination between samples.</li>
		</ol>
		</li>
		<li>Stack the plates in plastic bags, seal, and incubate upside down for 2-3 days at the same temperature used previously until single colonies become visible.</li>
	</ol>
	</li>
	<li>Identification of yeast species via ITS sequencing
	<ol>
		<li>Select a well-separated, single colony per soil isolate and subculture onto a fresh YEPD + chloramphenicol + benomyl plate to obtain more cells. Incubate for 2-3 days at the same temperature used previously.</li>
		<li>Harvest the freshly grown cells and suspend them in -80 &#176;C freezer tubes containing 1 mL of sterilized 30% glycerol in double-distilled water to create cell suspensions. Maintain these suspensions at -80 &#176;C as stock solutions.</li>
		<li>Use fresh cells to perform colony PCR (polymerase chain reaction) with primers ITS1 (5&#39; TCCGTAGGTGAACCTGCGG 3&#39;) and ITS4 (5&#39; TCCTCCGCTTATTGATATGC 3&#39;) to amplify the fungal barcoding gene, ITS9. Use the following thermocycling conditions: an initial denaturation step at 95 &#176;C for 10 min followed by 35 cycles of (i) 95 &#176;C for 30 s, (ii) 55 &#176;C for 30 s, and (iii) 72 &#176;C for 1 min. 
		NOTE: Colony PCR has a high success rate and a faster turnaround time than DNA extraction followed by PCR.</li>
		<li>If colony PCR repeatedly fails for a strain, extract DNA using the protocol of choice and perform ITS PCR using extracted genomic DNA as template (use same thermocycling conditions as above). 
		NOTE: A relatively inexpensive chloroform-based DNA extraction is recommended28.</li>
		<li>Perform Sanger sequencing to determine the DNA sequence of the amplified ITS region for each strain.</li>
		<li>Compare the obtained ITS sequence of the yeast strains to sequences deposited in public databases such as NCBI GenBank and UNITE to establish species identity.</li>
	</ol>
	</li>
</ol>
2. Isolation of Aspergillus fumigatus from soil
<ol>
	<li>Prepare 1 mL of sterile Sabouraud dextrose broth (SDB) supplemented with the antibiotic chloramphenicol per soil sample.
	<ol>
		<li>Add 10 g of peptone and 20 g of dextrose to 1 L of distilled water. Autoclave at 121 &#176;C for 40 min.</li>
		<li>Allow the SDB to cool to ~50 &#176;C, add 1 mL of 50 g/L chloramphenicol to bring the concentration to 50 mg/L. 
		NOTE: Chloramphenicol is prepared the same as described above for yeast isolation. Aside from inhibiting bacterial growth, chloramphenicol also prevents the production of gas from bacteria that will cause the tubes to open during the incubation step detailed in Step 2.2.</li>
		<li>Aseptically aliquot 1 mL of SDB into a 1.5 mL microcentrifuge tube per soil sample using a mechanical pipette.</li>
	</ol>
	</li>
	<li>Add soil to 1.5 mL microcentrifuge tubes.
	<ol>
		<li>Lay bench coat or absorbent padding inside a BSCII to aid in the disposal of spilt soil.</li>
		<li>Using autoclaved applicator sticks, transfer approximately 0.1 g of soil into a 1.5 mL microcentrifuge tube containing 1 mL of SBD. Close the tube and vortex. Incubate the suspended soil at 50 &#176;C for 3 days. 
		NOTE: Shaking during incubation is not required.</li>
	</ol>
	</li>
	<li>Mycelial harvest of soil-inoculated broth
	<ol>
		<li>Prepare malt extract agar (MEA) plates.
		<ol>
			<li>Per liter of MEA: add 20 g of malt extract, 20 g of dextrose, 6 g of peptone, and 15 g of agar to 1 L of distilled water. Autoclave at 121 &#176;C for 40 min.</li>
			<li>Allow the MEA to cool to ~50 &#176;C, then add 1 mL of 50 g/L chloramphenicol to bring to a final concentration of 50 mg/L.</li>
		</ol>
		</li>
		<li>Transfer the mycelia from the soil-inoculated broth onto MEA plates.
		<ol>
			<li>Identify soil inoculums that have visible mycelial growth at the SDB to air boundary.</li>
			<li>Use sterilized wooden plain-tipped applicator sticks to transfer the mycelia to the center of a MEA plate. Incubate the MEA plates at 37 &#176;C for 3 days.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Selection of mycelia with A. fumigatus morphological properties.
	<ol>
		<li>Identify mold colonies that have characteristic A. fumigatus morphological properties (green suede like growth).</li>
		<li>Working in a BSCII, use sterilized wooden plain-tipped applicator sticks or an inoculation loop to harvest conidia/mycelia by scraping the surface once. Transfer the spores/mycelia to the center of a MEA plate by streaking onto the agar for single colonies. Incubate at 37 &#176;C for 2 days. 
		NOTE: As multiple A. fumigatus strains and/or other fungi may be present on the plate, it is important to streak for single colonies. The single-colony streaking protocol in Step 1.5.3 in the yeast isolation protocol can be used.</li>
		<li>Using a sterile applicator stick or inoculation loop, subculture a single colony generated in Step 2.4.1.2 onto MEA by streaking the colony once. Spread the harvested spores into the center of the plate. Incubate at 37 &#176;C for 2 days.</li>
	</ol>
	</li>
	<li>Harvesting of A. fumigatus spores/mycelia for culture storage
	<ol>
		<li>Prepare a sterile 30% glycerol solution (for a 100 mL solution, add 30 mL of 100% glycerol mixed with 70 mL of double-distilled water, sterilized at 121 &#176;C for 40 min).</li>
		<li>Working in a BSCII, use a p1000 pipette to aspirate 1 mL of the 30% glycerol solution. Dispense the 1 mL of glycerol solution onto the A. fumigatus colony to harvest spores/mycelia.
		<ol>
			<li>Due to the hydrophobicity of A. fumigatus spores/mycelia, use the pipette tip to scratch a densely sporulated region of the plate. 
			NOTE: When glycerol is dispensed in the scratch, the glycerol would adhere to the scratch area rather than rolling over the agar.</li>
			<li>Slowly dispense the glycerol onto the scratch area to dislodge the spores and suspend them in the glycerol solution.</li>
			<li>Once fully dispensed, lightly tip the plate and aspirate the glycerol spore/mycelia suspension. 
			NOTE: Approximately 750 to 800 &#181;L will be aspirated.</li>
			<li>Transfer the aspirate to a sterile freezer tube and store at -80 &#176;C. If required, create working stock by repeating steps 2.5.2.1 to 2.5.2.4.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Phenotypic identification of A. fumigatus strains
	<ol>
		<li>Using the spore stock created from step 2.5.2, create a 100x dilution in water.
		<ol>
			<li>Aspirate 10 &#181;L of the mycelial and spore stocks and dispense in 990 &#181;L of water. Vortex the suspension.</li>
		</ol>
		</li>
		<li>Dispense 10 &#181;L of the diluted spore suspension onto a standard microscope slide.</li>
		<li>OPTIONAL: Stain the mycelial and spore suspension with methylene blue.
		<ol>
			<li>To stain with methylene blue, fix the conidia and conidiophores to the slide by passing the slide over a Bunsen burner until dry.</li>
			<li>Apply methylene blue for 1-2 min and wash off with water.</li>
			<li>Dry the slide with blotting paper.</li>
		</ol>
		</li>
		<li>Using a compound microscope at 400x magnification, view the suspension and locate conidiophores. Compare the observed conidiophore morphology with A. fumigatus conidiophore morphology.</li>
	</ol>
	</li>
	<li>Molecular identification of A. fumigatus strains
	<ol>
		<li>Extract DNA from each isolate following common fungal DNA extraction protocols.</li>
		<li>Using primers specific to the Aspergillus&#160;&#946;-tubulin genes (&#946;-tub1 and &#946;-tub4), run PCR and obtain the sequence for the amplified products, following protocols described by Alcazar-Fuoli et al.17.
		<ol>
			<li>Compare the obtained sequences to sequences deposited in public databases such as NCBI GenBank using BLAST.</li>
			<li>Confirm the strain sequences are a top match to A. fumigatus sequences in the database.</li>
		</ol>
		</li>
		<li>Alternative to step 2.7.2, run a multiplex PCR reaction targeting the A. fumigatus mating types MAT1-1 and MAT1-229.
		<ol>
			<li>Use the following three primer sequences in the multiplex PCR reaction: AFM1: 5&#39;-CCTTGACGCGATGGGGTGG-3&#39;; AFM2: 5&#8242;-CGCTCCTCATCAGAACAACTCG-3&#8242;; AFM3: 5&#8242;-CGGAAATCTGATGTCGCCACG-3&#8242;.</li>
			<li>Use the following thermocycler parameters: 5 min at 95 &#176;C, 35 cycles of 30 s at 95 &#176;C, 30 s at 60 &#176;C, and 1 min at 72 &#176;C before a final 5 min at 72 &#176;C.</li>
			<li>Run gel electrophoresis to identify the products; look for 834 bp MAT-1 or 438 bp MAT1-2. Use A. fumigatus strains that have confirmed mating type amplification as positive and negative controls.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Microsatellite genotyping of A. fumigatus strains through fragment analysis 
	NOTE: Although the steps listed below broadly cover genotyping A. fumigatus at nine microsatellite (STR) loci, only a few important considerations have been highlighted. For details on A. fumigatus STR genotyping, refer to De Valk et al.24,30.
	<ol>
		<li>Prepare three PCR multiplex master mixes using the STRAf primers previously described by De Valk et al.24.
		<ol>
			<li>Fluorescently label forward primers to determine fragment size through capillary electrophoresis. Ensure that the concentration of the forward primers is half (0.5 &#956;M) that of the reverse primers (1 &#956;M) within the master mix. 
			NOTE: For the best results, use fluorescent labels that have absorbance wavelengths that match those of the chosen dye standard used during capillary electrophoresis</li>
			<li>Use hot start polymerase for best results.</li>
			<li>Use a DNA concentration of 0.1 ng per reaction.</li>
		</ol>
		</li>
		<li>Run the multiplex PCR for each strain using the following PCR program: 95 &#176;C for 10 min, 40 cycles of 95 &#176;C for 30 s, 60 &#176;C for 30 s, and 72 &#176;C for 60 s, followed by 72 &#176;C for 10 min and a hold at 4 &#176;C.</li>
		<li>Check for amplified products through gel electrophoresis.</li>
		<li>Dilute the products to the desired level (typically ~50x) as recommended by fragment analyses specialists and run capillary electrophoresis. Perform three runs for each strain, with each run covering three multiplexed reactions with three different fluorescent probes.</li>
		<li>To determine the correct fragment size for each of the nine STR loci, use software capable of fragment analysis.
		<ol>
			<li>Retrieve the raw data obtained from capillary electrophoresis. Score the fragment sizes based on the largest peak using the fragment analysis software (e.g., Osiris).</li>
			<li>Convert the fragment sizes to repeat numbers for each of the nine loci. Use the fragment sizes of the repeat numbers of the reference strain Af293 as previously described by De Valk et al.24. 
			NOTE: Slight variations in fragment sizes may occur between different capillary electrophoresis platforms. Thus, it is important to include a common reference strain (and an internal ladder) with known fragment size for each of the nine loci for genotyping strains.</li>
		</ol>
		</li>
	</ol>
	</li>
</ol>

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A., 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=Use+of+a+novel+panel+of+nine+short+tandem+repeats+for+exact+and+high-resolution+fingerprinting+of+Aspergillus+fumigatus+isolates.">Use of a novel panel of nine short tandem repeats for exact and high-resolution fingerprinting of Aspergillus fumigatus isolates.</a> Journal of Clinical Microbiology. 43 (8), 4112-4120 (2005).</li><li>Yurkov, A. M., Kemler, M., Begerow, D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Assessment+of+yeast+diversity+in+soils+under+different+management+regimes.">Assessment of yeast diversity in soils under different management regimes.</a> Fungal Ecology. 5 (1), 24-35 (2012).</li><li>Calhelha, R. C., Andrade, J. V., Ferreira, I. C., Estevinho, L. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Toxicity+effects+of+fungicide+residues+on+the+wine-producing+process.">Toxicity effects of fungicide residues on the wine-producing process.</a> Food Microbiology. 23 (4), 393-398 (2006).</li><li>Thomas, J. H., Neff, N. F., Botstein, D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Isolation+and+characterization+of+mutations+in+the+&#914;-tubulin+gene+of+Saccharomyces+cerevisiae.">Isolation and characterization of mutations in the &#914;-tubulin gene of Saccharomyces cerevisiae.</a> Genetics. 111 (4), 715-734 (1985).</li><li>Xu, J., Ramos, A. R., Vilgalys, R., Mitchell, T. G. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Clonal+and+spontaneous+origins+of+fluconazole+resistance+in+Candida+albicans.">Clonal and spontaneous origins of fluconazole resistance in Candida albicans.</a> Journal of Clinical Microbiology. 38 (3), 1214 (2000).</li><li>Paoletti, M., 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=Evidence+for+sexuality+in+the+opportunistic+fungal+pathogen+Aspergillus+fumigatus.">Evidence for sexuality in the opportunistic fungal pathogen Aspergillus fumigatus.</a> Current Biology. 15 (13), 1242-1248 (2005).</li><li>De Valk, H. A., Meis, J. F. G. M., De Pauw, B. E., Donnelly, P. J., Klaassen, C. H. W. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Comparison+of+two+highly+discriminatory+molecular+fingerprinting+assays+for+analysis+of+multiple+Aspergillus+fumigatus+isolates+from+patients+with+invasive+aspergillosis.">Comparison of two highly discriminatory molecular fingerprinting assays for analysis of multiple Aspergillus fumigatus isolates from patients with invasive aspergillosis.</a> Journal of Clinical Microbiology. 45 (5), 1415-1419 (2007).</li><li>Bates, D., M&#228;chler, M., Bolker, B. M., Walker, S. C. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Fitting+linear+mixed-effects+models+using+lme4.">Fitting linear mixed-effects models using lme4.</a> Journal of Statistical Software. 67 (1), 1-48 (2015).</li><li>Camacho, C., Madden, T., Tao, T., Agarwala, R., Morgulis, A. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=BLAST+&#174;+Command+Line+Applications+User+Manual.">BLAST &#174; Command Line Applications User Manual.</a> National Center for Biotechnology Information. , 1-95 (2022).</li><li>Ashu, E. E., Korfanty, G. A., Xu, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Evidence+of+unique+genetic+diversity+in+Aspergillus+fumigatus+isolates+from+Cameroon.">Evidence of unique genetic diversity in Aspergillus fumigatus isolates from Cameroon.</a> Mycoses. 60 (11), 739-748 (2017).</li><li>Korfanty, G. A., Dixon, M., Jia, H., Yoell, H., Xu, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Genetic+diversity+and+dispersal+of+Aspergillus+fumigatus+in+Arctic+soils.">Genetic diversity and dispersal of Aspergillus fumigatus in Arctic soils.</a> Genes. 13 (1), 19 (2021).</li><li>Snelders, E., 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=Possible+environmental+origin+of+resistance+of+Aspergillus+fumigatus+to+medical+triazoles.">Possible environmental origin of resistance of Aspergillus fumigatus to medical triazoles.</a> Applied and Environmental Microbiology. 75 (12), 4053-4057 (2009).</li><li>Wang, H. -. C., 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=mechanisms+and+genetic+relatedness+of+the+human+pathogenic+fungus+Aspergillus+fumigatus+exhibiting+resistance+to+medical+azoles+in+the+environment+of+Taiwan.">mechanisms and genetic relatedness of the human pathogenic fungus Aspergillus fumigatus exhibiting resistance to medical azoles in the environment of Taiwan.</a> Environmental Microbiology. 20 (1), 270-280 (2018).</li></ol>

The authors have no conflicts of interest to declare.

The protocol developed for isolating yeasts and A. fumigatus from soil is a fast and efficient method for high-throughput soil processing and fungal isolation. The protocol only requires a small amount of soil (0.1-0.2 g) per sample, allowing for more sites to be sampled with similar effort. The quick turnaround time ensures that results can be obtained within a short timeframe and allows time for troubleshooting and repeating experiments if necessary. This protocol can be easily replicated across many laborator...

Fungi in soil ecosystems play essential roles in organic matter decomposition, nutrient cycling, and soil fertilization1. Both culture-independent (i.e., high-throughput sequencing) and culture-dependent approaches are widely used in the study of soil fungi2,3. While the large amount of data generated by high-throughput metabarcode sequencing is useful for elucidating broad-scale patterns in community structure and diversity, the culture-dependent approach can provide highly complementary information on the taxonomic and functional structures of fungal communities, as well as more specific profiles of individual organisms through downstream diversity and functional analyses due to the availability of pure fungal cultures.
Despite rarely exceeding thousands of cells per gram of soil, yeasts, broadly defined as unicellular fungi, are essential decomposers and food sources for other soil dwellers4,5. In fact, yeasts may be the predominant soil fungi in cold biospheres such as continental Antarctica6,7. Soil is also a primary reservoir of medically relevant yeasts that cause serious opportunistic infections in humans and other mammals8. Despite morphological similarities, yeast species are phylogenetically diverse and occur among filamentous fungi in two major phyla, Ascomycota and Basidiomycota, within the fungal kingdom9. Yeasts lack a defining DNA signature at the fungal barcoding gene, the internal transcribed spacer (ITS) region of the nuclear ribosomal RNA gene cluster10, making them indistinguishable from other fungi in metagenomics investigations and thus necessitating the use of culture-dependent methods to isolate yeast species.
The protocol below was implemented to characterize soil yeast communities of nine countries and identify global trends and patterns in soil yeast diversity9,11,12. Metagenomics approaches are of limited use when studying targeted groups of organisms such as yeasts2,3. Due to their phylogenetic diversity, yeasts cannot be distinguished from other fungi based on DNA sequence alone. Thus, studying yeast populations requires the continued use of culture-dependent isolation. However, culturing is often significantly more time-consuming and requires more personnel to perform the experiments. Therefore, the protocol has been optimized and streamlined for faster processing with limited personnel. The main advantage of culturing is that the yeast species identified are living yeasts and not dead ones, and thus are more likely to be true soil dwellers rather than transient cells present in the soils. It has been estimated that approximately 40% of fungal DNA in soil are either contaminants from other environments, extracellular, or come from cells that are no longer intact, causing high-throughput sequencing approaches to overestimate fungal richness by as much as 55%13. Culture-dependent isolation can readily confirm yeast species identity with the added benefit of securing pure culture to be used in downstream analyses. Indeed, pure cultures of 44 putative new yeast species were identified using this soil isolation protocol that allowed the use of a range of methods to study their taxonomic and functional properties in detail14.
The protocol below can also be used to isolate molds present within soil, such as A. fumigatus. Aspergillus fumigatus is a thermophilic and saprophytic mold with a wide, global distribution in soil15.&#160;It has been isolated from numerous clinical and non-clinical environments. Non-clinical sampling commonly includes air, organic debris (compost, saw dust, tulip bulb waste), and soil (agricultural, garden, and natural soils)16,17,18,19. Aspergillus fumigatus is a human opportunistic pathogen causing a range of infections collectively termed aspergillosis, affecting over 8 million people worldwide16,20. Approximately 300,000 people around the globe suffer from invasive aspergillosis, which is the most severe form of aspergillosis16. Depending on factors such as the patient population, site of infection, and efficacy of antifungal therapy, mortality rate can be as high as 90%. Over the past several decades, resistance to antifungal therapies has increased, requiring global surveillance efforts in both clinical and environmental populations to track these resistance genotypes21,22,23. Given its ability to grow at temperatures upward of 50 &#176;C, this temperature can be exploited to select for A. fumigatus isolates from soil using culture-dependent methods. Aspergillus fumigatus isolates are commonly genotyped at nine highly polymorphic short tandem repeat (STR) loci, shown to have high discriminatory power between strains24. These STR genotypes can be compared to other previously surveyed populations to track the spread of A. fumigatus genotypes, including drug-resistance genes, around the world.
Below we describe a protocol for the speedy isolation of yeasts and A. fumigatus from soil samples in a culture-dependent manner. Depending on the amount of soil obtained per sample, the soil samples can be shared between the two protocols. In comparison to similar methods that isolate yeast and A. fumigatus from soil, this protocol uses 10x less soil per isolate obtained. Studies attempting to isolate A. fumigatus from soil require between 1 and 2 g of soil per isolate, whereas this protocol requires only 0.1-0.2 g of soil18,19,25. This protocol utilizes smaller plastics and containers that facilitate its high-throughput design. Therefore, a larger number of samples can be processed using less space for equipment such as incubators and roller drums. Soil samples can be fully processed to obtain isolates in as little as 7 days. This protocol has been optimized to allow processing of up to 150-200 samples per day per person.

<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>1.5 mL microcentrifuge tube</td>
			<td>Sarstedt Inc</td>
			<td>72.690.001</td>
			<td></td>
		</tr>
		<tr>
			<td>Benomyl powder&#160;</td>
			<td>Toronto Research Chemicals</td>
			<td>B161380</td>
			<td></td>
		</tr>
		<tr>
			<td>Chloramphenicol powder&#160;</td>
			<td>Sigma-Aldrich</td>
			<td>SKU: C0378-5G</td>
			<td></td>
		</tr>
		<tr>
			<td>Dextrose</td>
			<td>Sigma-Aldrich</td>
			<td>SKU: D9434-500G</td>
			<td></td>
		</tr>
		<tr>
			<td>Fragment Analysis Software</td>
			<td>NCBI&#39;s Osiris</td>
			<td></td>
			<td>https://www.ncbi.nlm.nih.gov/osiris/</td>
		</tr>
		<tr>
			<td>ITS sequence database</td>
			<td>NCBI GenBank&#160;</td>
			<td></td>
			<td>https://www.ncbi.nlm.nih.gov/genbank/</td>
		</tr>
		<tr>
			<td>ITS sequence database</td>
			<td>UNITE&#160;</td>
			<td></td>
			<td>https://unite.ut.ee/</td>
		</tr>
		<tr>
			<td>Peptone</td>
			<td>Sigma-Aldrich</td>
			<td>SKU: P5905-500G</td>
			<td></td>
		</tr>
		<tr>
			<td>Reusable cell spreaders&#160;</td>
			<td>Fisher Scientific</td>
			<td>08-100-12</td>
			<td></td>
		</tr>
		<tr>
			<td>Sterile 10 cm diameter Petri dishes&#160;</td>
			<td>Sarstedt Inc</td>
			<td>83.3902</td>
			<td></td>
		</tr>
		<tr>
			<td>Sterile 13 mL culture tubes&#160;</td>
			<td>Sarstedt Inc</td>
			<td>62.515.006</td>
			<td></td>
		</tr>
		<tr>
			<td>Wooden plain-tipped applicator sticks&#160;</td>
			<td>Fisher Scientific</td>
			<td>23-400-112</td>
			<td></td>
		</tr>
		<tr>
			<td>Yeast extract</td>
			<td>Sigma-Aldrich</td>
			<td>SKU: Y1625-250G</td>
			<td></td>
		</tr>
	</tbody>
</table>

isolation of culturable yeasts and molds from soils to investigate fungal population structure

Soil is host to an incredible amount of microbial life, with each gram containing up to billions of bacterial, archaeal, and fungal cells. Multicellular fungi such as molds and unicellular fungi, broadly defined as yeasts, fulfill essential roles in soil ecosystems as decomposers of organic material and as food sources for other soil dwellers. Fungal species diversity in soil is dependent on a multitude of climatic factors such as rainfall and temperature, as well as soil properties including organic matter, pH, and moisture. Lack of adequate environmental sampling, especially in regions of Asia, Africa, South America, and Central America, hinders the characterization of soil fungal communities and the discovery of novel species. 
We characterized soil fungal communities in nine countries across six continents using ~4,000 soil samples and a protocol developed in the laboratory for the isolation of yeasts and molds. This protocol begins with separate selective enrichment for yeasts and the medically relevant mold Aspergillus fumigatus, in liquid media while inhibiting bacterial growth. Resulting colonies are then transferred to solid media and further processed to obtain pure cultures, followed by downstream genetic characterization. Yeast species identity is established via sequencing of their internal transcribed spacer (ITS) region of the nuclear ribosomal RNA gene cluster, while global population structure of A. fumigatus is explored via microsatellite marker analysis. 
The protocol was successfully applied to isolate and characterize soil yeast and A. fumigatus populations in Cameroon, Canada, China, Costa Rica, Iceland, Peru, New Zealand, and Saudi Arabia. These findings revealed much-needed insights on global patterns in soil yeast diversity, as well as global population structure and antifungal resistance profiles of A. fumigatus. This paper presents the method of isolating both yeasts and A. fumigatus from international soil samples.

Yeast isolation from soil 
The above yeast isolation protocol was implemented to culture yeasts from soil samples originating from 53 locations in nine countries9,12. In total, 1,473 yeast strains were isolated from 3,826 soil samples. Given the different climatic conditions of the nine originating countries, the best incubation temperature for each country was determined based on its mean annual temperature (Table 1). Given...

Watch this Scientific Journal Video about Isolation of Culturable Yeasts and Molds from Soils to Investigate Fungal Population Structure at JoVE.com

Isolation of Culturable Yeasts and Molds from Soils to Investigate Fungal Population Structure

This protocol is an effective, speedy method of culturing yeasts and the mold Aspergillus fumigatus from large sets of soil samples in as little as 7 days. The methods can be easily modified to accommodate a range of incubation media and temperatures as needed for experiments.

Soil is host to an incredible amount of microbial life, with each gram containing up to billions of bacterial, archaeal, and fungal cells. Multicellular ...

isolation-culturable-yeasts-molds-from-soils-to-investigate-fungal

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5.1K Views.  McMaster University. This protocol is an effective, speedy method of culturing yeasts and the mold Aspergillus fumigatus from large sets of soil samples in as little as 7 days. The methods can be easily modified to accommodate a range of incubation media and temperatures as needed for experiments. 

Video: Isolation of Culturable Yeasts and Molds from Soils to Investigate Fungal Population Structure

Extraction of High Molecular Weight Genomic DNA from Soils and Sediments

The soil microbiome is a vast and relatively unexplored reservoir of genomic diversity and metabolic innovation that is intimately associated with nutrient and energy flow within terrestrial ecosystems. Cultivation-independent environmental genomic, also known as metagenomic, approaches promise unprecedented access to this genetic information with respect to pathway reconstruction and functional screening for high value therapeutic and biomass conversion processes. However, the soil microbiome still remains a challenge largely due to the difficulty in obtaining high molecular weight DNA of sufficient quality for large insert library production. Here we introduce a protocol for extracting high molecular weight, microbial community genomic DNA from soils and sediments. The quality of isolated genomic DNA is ideal for constructing large insert environmental genomic libraries for downstream sequencing and screening applications. 
The procedure starts with cell lysis. Cell walls and membranes of microbes are lysed by both mechanical (grinding) and chemical forces (&beta;-mercaptoethanol). Genomic DNA is then isolated using extraction buffer, chloroform-isoamyl alcohol and isopropyl alcohol. The buffers employed for the lysis and extraction steps include guanidine isothiocyanate and hexadecyltrimethylammonium bromide (CTAB) to preserve the integrity of the high molecular weight genomic DNA. Depending on your downstream application, the isolated genomic DNA can be further purified using cesium chloride (CsCl) gradient ultracentrifugation, which reduces impurities including humic acids. The first procedure, extraction, takes approximately 8 hours, excluding DNA quantification step. The CsCl gradient ultracentrifugation, is a two days process. During the entire procedure, genomic DNA should be treated gently to prevent shearing, avoid severe vortexing, and repetitive harsh pipetting.

A methodology to isolate high molecular weight and high quality genomic DNA from soil microbial community is described.

The soil microbiome is a vast and relatively unexplored reservoir of genomic diversity and metabolic innovation that is intimately associated with ...

Isolation and Purification of Kinesin from Drosophila Embryos

Motor proteins move cargos along microtubules, and transport them to specific sub-cellular locations. Because altered transport is suggested to underlie a variety of neurodegenerative diseases, understanding microtubule based motor transport and its regulation will likely ultimately lead to improved therapeutic approaches. Kinesin-1 is a eukaryotic motor protein which moves in an anterograde (plus-end) direction along microtubules (MTs), powered by ATP hydrolysis. Here we report a detailed purification protocol to isolate active full length kinesin from Drosophila embryos, thus allowing the combination of Drosophila genetics with single-molecule biophysical studies. Starting with approximately 50 laying cups, with approximately 1000 females per cup, we carried out overnight collections. This provided approximately 10 ml of packed embryos. The embryos were bleach dechorionated (yielding approximately 9 grams of embryos), and then homogenized. After disruption, the homogenate was clarified using a low speed spin followed by a high speed centrifugation. The clarified supernatant was treated with GTP and taxol to polymerize MTs. Kinesin was immobilized on polymerized MTs by adding the ATP analog, 5'-adenylyl imidodiphosphate at room temperature. After kinesin binding, microtubules were sedimented via high speed centrifugation through a sucrose cushion. The microtubule pellet was then re-suspended, and this process was repeated. Finally, ATP was added to release the kinesin from the MTs. High speed centrifugation then spun down the MTs, leaving the kinesin in the supernatant. This kinesin was subjected to a centrifugal filtration using a 100 KD cut off filter for further purification, aliquoted, snap frozen in liquid nitrogen, and stored at -80 &deg;C. SDS gel electrophoresis and western blotting was performed using the purified sample. The motor activity of purified samples before and after the final centrifugal filtration step was evaluated using an in vitro single molecule microtubule assay. The kinesin fractions before and after the centrifugal filtration showed processivity as previously reported in literature. Further experiments are underway to evaluate the interaction between kinesin and other transport related proteins.

Isolation and Purification of Kinesin from Drosophila Embryos

This is a protocol to isolate active full length Kinesin from Drosophila embryos for single-molecule biophysical studies. We show how to collect embryos, make the embryo lysate, and then polymerize microtubules (MTs). Kinesin is purified by immobilizing it on the MTs, spinning down the Kinesin-MT complexes, and then releasing the kinesin from the MTs via ATP addition.

Motor proteins move cargos along microtubules, and transport them to specific sub-cellular locations. Because altered transport is suggested to underlie a ...

Isolation of Myofibroblasts from Mouse and Human Esophagus

Murine and human esophageal myofibroblasts are generated via enzymatic digestion. Neonate (8-12 day old) murine esophagus is harvested, minced, washed, and subjected to enzymatic digestion with collagenase and dispase for 25 min. Human esophageal resection specimens are stripped of muscularis propria and adventitia and the remaining mucosa is minced, and subjected to enzymatic digestion with collagenase and dispase for up to 6 hr. Cultured cells express &#945;-SMA and vimentin and express desmin weakly or not at all. Culture conditions are not conducive to growth of epithelial, hematopoietic, or endothelial cells. Culture purity is further confirmed by flow cytometric evaluation of cell surface marker expression of potential contaminating hematopoietic and endothelial cells. The described technique is straightforward and results in consistent generation of non-hematopoieitc, non-endothelial stromal cells. Limitations of this technique are inherent to the use of primary cultures in molecular biology studies, i.e., the unavoidable variability encountered among cultures established across different mice or humans. Primary cultures however are a more representative reflection of the in vivo state compared to cell lines. These methods also provide investigators the ability to isolate and culture stromal cells from different clinical and experimental conditions, allowing comparisons between groups. Characterized esophageal stromal cells can also be used in functional studies investigating epithelial-stromal interactions in esophageal disorders.

We present a protocol to generate primary cultures of murine and human esophageal stromal cells with a myofibroblast phenotype. Cultured cells have spindle shaped morphology, express &#945;-SMA and vimentin, and lack epithelial, hematopoietic and endothelial cell surface markers. Characterized stromal cells can be used in functional studies of epithelial-stromal interactions.

Murine and human esophageal myofibroblasts are generated via enzymatic digestion. Neonate (8-12 day old) murine esophagus is harvested, minced, washed, ...

Analysis of Autophagy in Penicillium chrysogenum by Using Starvation Pads in Combination With Fluorescence Microscopy

The study of cellular quality control systems has emerged as a highly dynamic and relevant field of contemporary research. It has become clear that cells possess several lines of defense against damage to biologically relevant molecules like nucleic acids, lipids and proteins. In addition to organelle dynamics (fusion/fission/motility/inheritance) and tightly controlled protease activity, the degradation of surplus, damaged or compromised organelles by autophagy (cellular &#8216;self-eating&#8217;) has received much attention from the scientific community. The regulation of autophagy is quite complex and depends on genetic and environmental factors, many of which have so far not been elucidated. Here a novel method is presented that allows the convenient study of autophagy in the filamentous fungus Penicillium chrysogenum. It is based on growth of the fungus on so-called &#8216;starvation pads&#8217; for stimulation of autophagy in a reproducible manner. Samples are directly assayed by microscopy and evaluated for autophagy induction / progress. The protocol presented here is not limited for use with P. chrysogenum and can be easily adapted for use in other filamentous fungi.

Analysis of Autophagy in Penicillium chrysogenum by Using Starvation Pads in Combination With Fluorescence Microscopy

A convenient and powerful method for studying autophagy in Penicillium chrysogenum by using starvation pads (mixtures of agarose and tap water in a microscope slide containing a central cavity) is presented here.

The study of cellular quality control systems has emerged as a highly dynamic and relevant field of contemporary research. It has become clear that cells ...

Removal of Exogenous Materials from the Outer Portion of Frozen Cores to Investigate the Ancient Biological Communities Harbored Inside

The cryosphere offers access to preserved organisms that persisted under past environmental conditions. In fact, these frozen materials could reflect conditions over vast time periods and investigation of biological materials harbored inside could provide insight of ancient environments. To appropriately analyze these ecosystems and extract meaningful biological information from frozen soils and ice, proper collection and processing of the frozen samples is necessary. This is especially critical for microbial and DNA analyses since the communities present may be so uniquely different from modern ones. Here, a protocol is presented to successfully collect and decontaminate frozen cores. Both the absence of the colonies used to dope the outer surface and exogenous DNA suggest that we successfully decontaminated the frozen cores and that the microorganisms detected were from the material, rather than contamination from drilling or processing the cores.

The cryosphere offers access to preserved organisms that persisted under past environmental conditions. A protocol is presented to collect and decontaminate permafrost cores of soils and ice. The absence of exogenous colonies and DNA suggest that microorganisms detected represent the material, rather than contamination from drilling or processing.

The cryosphere offers access to preserved organisms that persisted under past environmental conditions. In fact, these frozen materials could reflect ...

Isolation and Characterization of Microvesicles from Peripheral Blood

The release of extracellular vesicles (EVs) including small endosomal-derived exosomes (Exos, diameter &#60; 100 nm) and large plasma membrane-derived microvesicles (MVs, diameter &#62; 100 nm) is a fundamental cellular process that occurs in all living cells. These vesicles transport proteins, lipids and nucleic acids specific for their cell of origin and in vitro studies have highlighted their importance as mediators of intercellular communication. EVs have been successfully isolated from various body fluids and especially EVs in blood have been identified as promising biomarkers for cancer or infectious diseases. In order to allow the study of MV subpopulations in blood, we present a protocol for the standardized isolation and characterization of MVs from peripheral blood samples. MVs are pelleted from EDTA-anticoagulated plasma samples by differential centrifugation and typically possess a diameter of 100 - 600 nm. Due to their larger size, they can easily be studied by flow cytometry, a technique that is routinely used in clinical diagnostics and available in most laboratories. Several examples for quality control assays of the isolated MVs will be given and markers that can be used for the discrimination of different MV subpopulations in blood will be presented.

Extracellular vesicles present in blood have been suggested as novel biomarkers for various diseases. Here, we present a protocol for the isolation of large plasma membrane-derived microvesicles from peripheral blood samples and their subsequent analysis by conventional flow cytometry and Western Blotting.

The release of extracellular vesicles (EVs) including small endosomal-derived exosomes (Exos, diameter &#60; 100 nm) and large plasma membrane-derived ...

Techniques to Induce and Quantify Cellular Senescence

In response to cellular stress or damage, proliferating cells can induce a specific program that initiates a state of long-term cell-cycle arrest, termed cellular senescence. Accumulation of senescent cells occurs with organismal aging and through continual culturing in vitro. Senescent cells influence many biological processes, including embryonic development, tissue repair and regeneration, tumor suppression, and aging. Hallmarks of senescent cells include, but are not limited to, increased senescence-associated &#946;-galactosidase activity (SA-&#946;-gal); p16INK4A, p53, and p21 levels; higher levels of DNA damage, including &#947;-H2AX; the formation of Senescence-associated Heterochromatin Foci (SAHF); and the acquisition of a Senescence-associated Secretory Phenotype (SASP), a phenomenon characterized by the secretion of a number of pro-inflammatory cytokines and signaling molecules. Here, we describe protocols for both replicative and DNA damage-induced senescence in cultured cells. In addition, we highlight techniques to monitor the senescent phenotype using several senescence-associated markers, including SA-&#946;-gal, &#947;-H2AX and SAHF staining, and to quantify protein and mRNA levels of cell cycle regulators and SASP factors. These methods can be applied to the assessment of senescence in various models and tissues.

Cellular senescence, the irreversible state of cell-cycle arrest, can be induced by various cellular stresses. Here, we describe protocols to induce cellular senescence and methods to assess markers of senescence.

In response to cellular stress or damage, proliferating cells can induce a specific program that initiates a state of long-term cell-cycle arrest, termed ...

Live-cell Imaging of Fungal Cells to Investigate Modes of Entry and Subcellular Localization of Antifungal Plant Defensins

Small cysteine-rich defensins are one of the largest groups of host defense peptides present in all plants. Many plant defensins exhibit potent in vitro antifungal activity against a broad-spectrum of fungal pathogens and therefore have the potential to be used as antifungal agents in transgenic crops. In order to harness the full potential of plant defensins for diseases control, it is crucial to elucidate their mechanisms of action (MOA). With the advent of advanced microscopy techniques, live-cell imaging has become a powerful tool for understanding the dynamics of the antifungal MOA of plant defensins. Here, a confocal microscopy based live-cell imaging method is described using two fluorescently labeled plant defensins (MtDef4 and MtDef5) in combination with vital fluorescent dyes. This technique enables real-time visualization and analysis of the dynamic events of MtDef4 and MtDef5 internalization into fungal cells. Importantly, this assay generates a wealth of information including internalization kinetics, mode of entry and subcellular localization of these peptides. Along with other cell biological tools, these methods have provided critical insights into the dynamics and complexity of the MOA of these peptides. These tools can also be used to compare the MOA of these peptides against different fungi.

Plant defensins play an important role in plant defense against pathogens. For effective use of these antifungal peptides as antifungal agents, understanding their modes of action (MOA) is critical. Here, a live-cell imaging method is described to study critical aspects of the MOA of these peptides.

Small cysteine-rich defensins are one of the largest groups of host defense peptides present in all plants. Many plant defensins exhibit potent in vitro ...

Sequential Immunofluorescence and Immunohistochemistry on Cryosectioned Zebrafish Embryos

Investigation of intercellular interactions often requires discrete labeling of specific cell populations and precise protein localization. The zebrafish embryo is an excellent tool for examining such interactions with an in vivo model. Whole-mount immunohistochemical and immunofluorescence assays are frequently applied in zebrafish embryos to assess protein expression. However, it can be difficult to achieve accurate mapping of co-localized proteins in three-dimensional space. In addition, some studies may require the use of two antibodies that are not compatible with the same technique (e.g., antibody 1 is only suitable for immunohistochemistry and antibody 2 is only suitable for immunofluorescence). The purpose of the method described herein is to perform sequential immunofluorescence and/or immunohistochemistry on individual cryosections derived from early-stage zebrafish embryos. Here we describe the use of sequential rounds of immunofluorescence, imaging, immunohistochemistry, imaging for a single cryosection in order to achieve precise identification of protein expression at the single-cell level. This methodology is suitable for any study in early-stage zebrafish embryos that requires accurate identification of multiple protein targets in individual cells.

This protocol demonstrates sequential immunofluorescence and immunohistochemistry on cryosections from early-stage zebrafish embryos enabling precise colocalization analyses in specific cell populations.

Investigation of intercellular interactions often requires discrete labeling of specific cell populations and precise protein localization. The zebrafish ...

Isolation of High Quality Murine Atrial and Ventricular Myocytes for Simultaneous Measurements of Ca2+ Transients and L-Type Calcium Current

Mouse models play a crucial role in arrhythmia research and allow studying key mechanisms of arrhythmogenesis including altered ion channel function and calcium handling. For this purpose, atrial or ventricular cardiomyocytes of high quality are necessary to perform patch-clamp measurements or to explore calcium handling abnormalities. However, the limited yield of high-quality cardiomyocytes obtained by current isolation protocols does not allow both measurements in the same mouse. This article describes a method to isolate high-quality murine atrial and ventricular myocytes via retrograde enzyme-based Langendorff perfusion, for subsequent simultaneous measurements of calcium transients and L-type calcium current from one animal. Mouse hearts are obtained, and the aorta is rapidly cannulated to remove blood. Hearts are then initially perfused with a calcium-free solution (37 &#176;C) to dissociate the tissue at the level of intercalated discs and afterwards with an enzyme solution containing little calcium to disrupt extracellular matrix (37 &#176;C). The digested heart is subsequently dissected into atria and ventricles. Tissue samples are chopped into small pieces and dissolved by carefully pipetting up and down. The enzymatic digestion is stopped, and cells are stepwise reintroduced to physiologic calcium concentrations. After loading with a fluorescent Ca2+-indicator, isolated cardiomyocytes are prepared for simultaneous measurement of calcium currents and transients. Additionally, isolation pitfalls are discussed and patch-clamp protocols and representative traces of L-type calcium currents with simultaneous calcium transient measurements in atrial and ventricular murine myocytes isolated as described above are provided.

Isolation of High Quality Murine Atrial and Ventricular Myocytes for Simultaneous Measurements of Ca2+ Transients and L-Type Calcium Current

Mouse models allow studying key mechanisms of arrhythmogenesis. For this purpose, high quality cardiomyocytes are necessary to perform patch-clamp measurements. Here, a method to isolate murine atrial and ventricular myocytes via retrograde enzyme-based Langendorff perfusion, which allows simultaneous measurements of calcium-transients and L-type calcium current, is described.

Mouse models play a crucial role in arrhythmia research and allow studying key mechanisms of arrhythmogenesis including altered ion channel function and ...