The authors wish to thank Anne Tanner, Bruce Paster, Heike Boisvert, Xuesong He and Batbileg Bor for helpful discussions and for providing bacterial strains. We thank Susan Yost and Jessica Woods for microbial technical assistance. Research reported in this publication was supported by The National Institute of Dental and Craniofacial Research of the National Institutes of Health under award numbers R37 DE016937 (FED), R01 DE024468 (FED) and T32 DE007327 (AJC). The content is solely the responsibility of the authors and does not necessarily represent the official views of the National Institutes of Health.

When developing this protocol, IRB approval was sought and approved (#14-10) and informed consent was obtained from all subjects.
1. Preparation
<ol>
	<li>When working with human subjects, obtain necessary IRB approval and informed consent.</li>
	<li>Start cultures of host bacteria with enough time to grow to early stationary phase. For example, inoculate 2-5 mL of tryptic soy broth with 0.1% yeast extract added (TSBY)&#160;with Arachnia propionica and incubate at 37 &#176;C for 24 h.</li>
	<li>Assemble filter holders with track-etched 0.2 &#181;m filter membrane. Wrap the assembly in foil and sterilize by autoclaving.</li>
	<li>Sterilize centrifuge tubes and cap assemblies.</li>
</ol>
2. Obtain sample of oral bacteria
NOTE: While many oral samples contain Saccharibacteria (e.g., saliva, swabs of tonsils, tongue scrapings) dental plaque routinely is the most successful.
<ol>
	<li>Take a plaque scraping using a sterile paper point, Gracey curette, or, if self-sampling, use a sterile toothpick or pipette tip. Transfer plaque to a suitable buffer, such as maximal recovery diluent (MRD, 0.85% NaCl, 0.1% peptone) or PBS. If not processed immediately, keep the sample on ice until ready to proceed.</li>
	<li>Vigorously resuspend the dental plaque in MRD buffer using a combination of vortexing and pipetting with a small pipet tip.</li>
	<li>Add resuspended plaque sample to an additional 9 mL of MRD buffer.</li>
</ol>
3. Prepare filtrate from oral sample
<ol>
	<li>Using aseptic technique, unwrap a sterile filter assembly. Untwist a quarter turn and retighten the filter holder to be sure threads are properly engaged and the apparatus is closed properly. Using a syringe, wash the membrane by passing 10 mL of MRD buffer through the apparatus. Improper assembly is revealed at this step by fluid leaking out of the filter holder. If leakage occurs, obtain another sterile filter assembly and repeat the wash step.</li>
	<li>Apply the sample to the washed filter. Remove the plunger from a syringe and attach it to the filter apparatus. Pour the dispersed dental sample, now in 10 mL of MRD buffer, into a syringe and load it onto the filter.</li>
	<li>Place a sterile centrifuge tube beneath the filter apparatus to catch the filtrate, then apply light pressure to the plunger to push the sample through the filter.</li>
	<li>Repeat the procedure with another 10 mL of MRD buffer to wash the membrane, collecting the flow-through in the same tube as the filtered sample. Aseptically cap the tube.</li>
</ol>
4. Concentrate Saccharibacteria cells by centrifugation
<ol>
	<li>Make an orientation mark on the tube and cap and place the tube in a high-speed centrifuge with the mark on the upper side. The pellet formed from centrifugation is usually invisible. The marking will help determine where the pellet of Saccharibacteria cells is located when centrifugation is done and the tube removed from the centrifuge.</li>
	<li>Centrifuge the samples at 60,000 x g for 1 h at 4 &#176;C. 
	NOTE: This force and time is sufficient to pellet all Saccharibacteria cells. However, Saccharibacteria cells can be at least partially pelleted by centrifuging for as little as 20 min at 20,000 x g.</li>
	<li>Carefully remove the tubes from centrifuge. Pour out the liquid from the tube, keeping the pellet on the upper side of the tube.</li>
	<li>Resuspend the usually invisible pellet in 1-2 mL of MRD buffer by vigorous vortexing.</li>
</ol>
5. Infect host cultures with Saccharibacteria-enriched filtrate
<ol>
	<li>Prepare culture tubes by aliquoting 2 mL of appropriate growth media (e.g., TSBY, BHI, etc.) into tubes.</li>
	<li>Add 200 &#181;L of overnight culture of host organisms to each tube. Add 100-200 &#181;L of resuspended, filtered sample to each tube.</li>
	<li>Incubate combined samples as appropriate for the host organism (e.g., 37 &#176;C, in an aerobic atmosphere for A. propionica).</li>
	<li>Passage the cells every two to three days by transferring 200 &#181;L of binary culture to 2 mL of fresh growth medium in a new tube. If it appears that the passaged cultures show no growth (i.e., the turbidity/optical density of the culture doesn&#39;t increase after passage into fresh media) the Saccharibacteria could be overwhelming or killing all the host organism. To remedy this, add 200 &#181;L of uninfected host culture when passaging the cells. Repeat for at least 5 passages.</li>
</ol>
6. Confirm infection by PCR
<ol>
	<li>After 5 passages, confirm infection with PCR. Five passages will ensure than any non-growing Saccharibacteria cells have been depleted beyond the limit of detection using 25 cycles of PCR.</li>
	<li>Prepare a PCR mastermix. A suggested recipe using is as follows, for each tube needed, prepare 12.5 &#181;L 2x PCR buffer, 0.75 &#181;L 10 &#181;M Forward primer (580F12 - AYT GGG CGT AAA GAG TTG C), 0.75 &#181;L 10 &#181;M Reverse primer (1177R13- GAC CTG ACA TCA TCC CCT CCT TCC), 1 &#181;L 25 mM MgCl2 and 9 &#181;L water. Mix by vortexing.</li>
	<li>Aliquot 24 &#181;L of mastermix into a 0.2 mL PCR tube. Add 1 &#181;L of Saccharibacteria-infected culture to the PCR reaction. Place the tube in a thermocycler and perform the following protocol: Initial denaturation 95 &#176;C for 5 min, 25 cycles of 95 &#176;C for 30 s, 60 &#176;C for 30 s, 72 &#176;C for 30 s, final elongation at 72 &#176;C for 2 min, then final hold at 4 &#176;C.</li>
	<li>Load and run the PCR products in a 1% agarose gel. A band of ~600 bases will indicate the presence of Saccharibacteria.</li>
</ol>
7. Check for purity and remove contaminating organisms
<ol>
	<li>Confirm purity of positive cultures by plating the coculture of Saccharibacteria on nutrient agar sufficient for the growth of the host organism. Perform a 10-fold serial dilution of the culture in sterile buffer (e.g., MRD or PBS) and spread 100 &#181;L on an agar plate. Perform dilutions such that there will be approximately 20-200 colonies growing on the agar plate.</li>
	<li>Incubate the culture in appropriate growth conditions and observe for contaminating organisms. 
	NOTE: Axenic Saccharibacteria colonies have never been observed, so only the host organism is observed growing on these plates. More than one colony type usually indicates contamination. Should contamination occur, the culture should be re-filtered to remove the unwanted contaminants and re-inoculated onto fresh host.</li>
	<li>Occasionally a double infection occurs, where two Saccharibacteria species infect the same host. To separate the Saccharibacteria species, resuspend individual colonies in 20 &#181;L sterile PBS and use 1 &#181;L of suspension in a PCR reaction to detect colonies with Saccharibacteria infections.</li>
	<li>Transfer the suspensions that gave a positive result to growth medium to start a binary culture. The success rate will depend on the titer of each Saccharibacteria species in the culture. It may be necessary to screen more than 50 colonies to find an infected one for propagation.</li>
</ol>
8. Storage of cultures
<ol>
	<li>Grow a binary culture of sufficient volume (10-50 mL) overnight.</li>
	<li>Pellet cells by centrifugation (4,000 x g for 10 min). 
	NOTE: High-speed centrifugation is not necessary here as Saccharibacteria cells will be attached to the larger, heavier cells of the host and will pellet with them.</li>
	<li>Resuspend cells in cryoprotectant. Growth media supplemented with either 5% DMSO or 20% glycerol is usually sufficient. Ensure that the host organism is compatible with cryoprotectant media (e.g., Growth of A. propionica is inhibited by glycerol and frozen stocks may not revive). Test the viability of an uninfected host culture with cryoprotectant to ensure stocks can survive freezing.</li>
	<li>Resuspend cell pellet in the same volume of culture (10-50 mL). Aliquot 0.5 mL into labeled cryovials. Freeze cell cultures at -80 &#176;C.</li>
</ol>

<ol>
	<li>Stewart, E. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Growing+unculturable+bacteria.">Growing unculturable bacteria.</a> Journal of Bacteriology. 194 (16), 4151-4160 (2012).</li><li>Bomar, L., Maltz, M., Colston, S., Graf, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Directed+culturing+of+microorganisms+using+metatranscriptomics.">Directed culturing of microorganisms using metatranscriptomics.</a> mBio. 2 (2), 00012 (2011).</li><li>Derrien, M., Vaughan, E. E., Plugge, C. M., de Vos, W. M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Akkermansia+muciniphila+gen.+nov.,+sp.+nov.,+a+human+intestinal+mucin-degrading+bacterium.">Akkermansia muciniphila gen. nov., sp. nov., a human intestinal mucin-degrading bacterium.</a> International Journal of Systematic and Evolutionary Microbiology. 54, 1469-1476 (2004).</li><li>Nelson, M. C., Bomar, L., Maltz, M., Graf, J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Mucinivorans+hirudinis+gen.+nov.,+sp.+nov.,+an+anaerobic,+mucin-degrading+bacterium+isolated+from+the+digestive+tract+of+the+medicinal+leech+Hirudo+verbana.">Mucinivorans hirudinis gen. nov., sp. nov., an anaerobic, mucin-degrading bacterium isolated from the digestive tract of the medicinal leech Hirudo verbana.</a> International Journal of Systematic and Evolutionary Microbiology. 65, 990-995 (2015).</li><li>Scott, J. C., Klein, B. A., Duran-Pinedo, A., Hu, L., Duncan, M. J. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+two-component+system+regulates+hemin+acquisition+in+porphyromonas+gingivalis.">A two-component system regulates hemin acquisition in porphyromonas gingivalis.</a> PLoS One. 8 (9), 0073351 (2013).</li><li>Martin, B., 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=New+growth+media+for+oral+bacteria.">New growth media for oral bacteria.</a> Journal of Microbiological Methods. 153 (22), 10-13 (2018).</li><li>Vartoukian, S. R., 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=In+vitro+cultivation+of+'unculturable'+oral+bacteria,+facilitated+by+community+culture+and+media+supplementation+with+siderophores.">In vitro cultivation of 'unculturable' oral bacteria, facilitated by community culture and media supplementation with siderophores.</a> Plos One. 11 (1), 0146926 (2016).</li><li>Strandwitz, 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=GABA-modulating+bacteria+of+the+human+gut+microbiota.">GABA-modulating bacteria of the human gut microbiota.</a> Nature Microbiology. 4 (3), 396-403 (2019).</li><li>Hug, L. 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=A+new+view+of+the+tree+of+life.">A new view of the tree of life.</a> Nature Microbiology. 1, 16048 (2016).</li><li>Castelle, C. J., Banfield, J. F. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Major+new+microbial+groups+expand+diversity+and+alter+our+understanding+of+the+tree+of+life.">Major new microbial groups expand diversity and alter our understanding of the tree of life.</a> Cell. 172 (6), 1181-1197 (2018).</li><li>He, X., 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=Cultivation+of+a+human-associated+TM7+phylotype+reveals+a+reduced+genome+and+epibiotic+parasitic+lifestyle.">Cultivation of a human-associated TM7 phylotype reveals a reduced genome and epibiotic parasitic lifestyle.</a> Proceedings of the National Academy of Sciences of the United States of America. 112 (1), 244-249 (2015).</li><li>Hugenholtz, P., Tyson, G., Webb, R. I., Wagner, A. M., Blackall, L. L. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Investigation+of+candidate+division+TM7,+a+recently+recognized+major+lineage+of+the+domain+Bacteria+with+no+known+pure-culture+representatives.">Investigation of candidate division TM7, a recently recognized major lineage of the domain Bacteria with no known pure-culture representatives.</a> Applied and Environmental Microbiology. 67 (1), 411-419 (2001).</li><li>Brinig, M., Lepp, P. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Prevalence+of+bacteria+of+division+TM7+in+human+subgingival+plaque+and+their+association+with+disease.">Prevalence of bacteria of division TM7 in human subgingival plaque and their association with disease.</a> Applied and Environmental Microbiology. 69 (3), 1687-1694 (2003).</li><li>Bor, B., 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=Insights+obtained+by+culturing+saccharibacteria+with+their+bacterial+hosts.">Insights obtained by culturing saccharibacteria with their bacterial hosts.</a> Journal of Dental Research. , 689-694 (2020).</li><li>Bor, B., 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=Phenotypic+and+physiological+characterization+of+the+epibiotic+interaction+between+TM7x+and+its+basibiont+actinomyces.">Phenotypic and physiological characterization of the epibiotic interaction between TM7x and its basibiont actinomyces.</a> Microbial Ecology. 71 (1), 243-255 (2016).</li><li>Skopek, R. J., Liljemark, W. F., Bloomquist, C. G., Rudney, J. D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Dental+plaque+development+on+defined+streptococcal+surfaces.">Dental plaque development on defined streptococcal surfaces.</a> Oral Microbiology and Immunology. 8 (1), 16-23 (1993).</li><li>Murugkar, P. P., Collins, A. J., Chen, T., Dewhirst, F. E. <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+cultivation+of+candidate+phyla+radiation+Saccharibacteria+(TM7)+bacteria+in+coculture+with+bacterial+hosts.">Isolation and cultivation of candidate phyla radiation Saccharibacteria (TM7) bacteria in coculture with bacterial hosts.</a> Journal of Oral Microbiology. 12 (1), 1814666 (2020).</li><li>Cross, K. L., 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=Targeted+isolation+and+cultivation+of+uncultivated+bacteria+by+reverse+genomics.">Targeted isolation and cultivation of uncultivated bacteria by reverse genomics.</a> Nature Biotechnology. 37 (11), 1314-1321 (2019).</li><li>Kantor, R., 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=Small+genomes+and+sparse+metabolisms+of+sediment-associated+bacteria+from+four+candidate+phyla.">Small genomes and sparse metabolisms of sediment-associated bacteria from four candidate phyla.</a> MBio. 4 (5), 00708-00713 (2013).</li></ol>

The authors have nothing to disclose.

Our method of filtering plaque and applying it to pure cultures of host organisms is largely based on earlier observations on the first cultured Saccharibacteria, &#39;Nanosynbacter lyticus&#39; strain TM7x11,14,15. Given the small cell size, we deduced that they could be separated from dental plaque using a filter and concentrated with centrifugation. Second, as these organisms live as parasites, providing these cells pure cultures of hosts would allow them to enter into a symbiosis and grow as binary cultures.
One advantage of this method is that it does not require an enrichment culture or selective pressure. &#39;Nanosynbacter lyticus&#39; strain TM7x was cultured from an enrichment culture using streptomycin as a selective agent, which sequencing had suggested would be effective at enriching for Saccharibacteria. Fortuitously, the host for &#39;Nanosynbacter lyticus&#39; Schaalia odontolytica, is known to be resistant to streptomycin16. Using antibiotics as a selective agent could also prevent the host organism from growing, which in turn would preclude the growth of Saccharibacteria.
A larger issue of using enrichment cultures is that fast-growing organisms will quickly displace organisms of interest. In the oral cavity, for example, Streptococcus species can grow quickly and, if sugar is present in the growth medium, produce enough acid to acidify the medium, further selecting against organisms of interest. By avoiding an enrichment culture and selective antibiotics, our method provides a general approach that could be applied to a wider range of Saccharibacteria and potential hosts without the complications of these other methods.
There are some obstacles to the method presented here. First, this method assumes that Saccharibacteria live in a binary culture. We have not tested combinations of trinary or ternary cultures to gauge their effectiveness, but there are likely Saccharibacteria that require growth factors that a single host organism cannot supply. Testing the vast combinations of oral bacteria that could support the growth of Saccharibacteria would be a daunting task. Second, the method assumes all Saccharibacteria are small enough to pass through a 0.2 &#181;m filter. It could be that other Saccharibacteria are larger than believed and the filter is selecting against these organisms. A filter with a larger pore size could be used, but this runs the risk of allowing more unwanted oral bacteria into the infected co-culture. Lastly, it is very difficult to find host species outside of those that have already been published. Thus far, the only successful hosts are species from the genera Actinomyces, Schaalia, Arachnia and Cellulosimicrobium, all members of the phylum Actinobacteria15,17,18. However, these hosts only support the growth of specific Saccharibacteria. To culture more species of Saccharibacteria, many more hosts must be explored.
We hope the method presented here will aid future research of the Saccharibacteria and other CPR organisms. Metagenomic sequencing suggests that these organisms also have small genomes and are suspected to be symbionts or rely on the local microbial community to supply metabolites and other factors critical to their survival19. A similar filtering strategy could be used to isolate these organisms, provided they are small enough and that their host organisms(s) can be cultured. The methods described here are a first step to bringing the powerful tools of laboratory culture to this large and diverse group of bacteria.

Culturing novel species of bacteria and bringing them into the laboratory allows for powerful experiments to better understand their physiology and broader interactions within their microbial community. While there are culture-free methods of interrogating these questions (e.g., &#34;meta-omics&#34;), the complex interactions of diverse microbial populations make it difficult to tease apart single variables and reach meaningful conclusions. While culturing bacteria has many benefits, there are many potential barriers to isolating a bacterium and growing it in pure culture. Potential specific growth requirements include pH, oxygen tension, vitamins, growth factors, signaling molecules or even direct cell contact to elicit growth1. However, it is believed that specific auxotrophies are the primary deterrent to culturing new species of bacteria. Standard media formulations lack many nutrients required by uncultivated bacteria, such as specific vitamins or carbons sources. These missing molecules can be key to the physiology of the uncultured bacteria and are usually provided by either another organism in the microbial community or a host organism. For example, complex carbohydrates such as mucins can be provided by animal hosts. Adding these to media has allowed cultivation of several bacteria from animal guts, including Akkermansia muciniphila and Mucinivorans hirudinis2,3,4. Many pathogenic bacteria have evolved the ability to use iron bound to hemin in animal cells, including the oral pathogen Porphyromonas gingivalis5. In the laboratory, the growth of Porphyromonas and other organisms, can be stimulated by the addition of hemin6.
Recently, many breakthroughs in culturing novel isolates of bacteria have come through co-culturing, using a &#34;feeder&#34; organism to provide specific factors to uncultured bacteria necessary for their growth. An elegant study by Vartoukian and colleagues showed that siderophores, iron binding molecules produced by bacteria, stimulated the growth of several novel oral isolates. Pyoverdines, a type of siderophore produced by pseudomonad species, were shown to significantly facilitate the growth of a novel Prevotella species7. In the same study, the first oral isolate for the phylum Chloroflexi was cultivated, also using F. nucleatum as a helper for providing some as yet unknown compound7. More recently, a bacterium from the genus Ruminococcaceae was isolated using Bacteroides fragilis as helper organism8. It was later shown that gamma aminobutyric acid (GABA), an inhibitory neurotransmitter, was required for growth on laboratory media. Using feeder organisms has proved to be a key strategy to mimicking specific microenvironments where uncultured bacteria grow, being more efficient than continuously reformulating growth media with different additives in varying concentrations.
One of the largest groups of uncultured bacteria are in the &#34;Candidate Phyla Radiation&#34; (CPR), a monophyletic group of several candidate bacterial phyla9,10. As of this writing, only members of the Saccharibacteria phylum within the CPR have been successfully cultured in the laboratory. The first isolate, &#39;Nanosynbacter lyticus&#39; strain TM7x, was isolated using the antibiotic streptomycin, which had been predicted to enrich for the uncultured TM711,12. A key discovery of this work was that the new isolate grew as a parasite growing in direct contact with a bacterial host, Schaalia odontolytica, and microscopy showed these parasites were ultrasmall bacteria.
Using these clues, we devised a method to quickly establish binary cocultures of Saccharibacteria with their partners by filtering dental plaque and other oral samples through a 0.2 &#181;m filter, collecting cells in the filtrate by centrifugation and using them to infect cultures of candidate host bacteria. This method has the advantage of avoiding enrichment cultures, which can be overwhelmed with fast-growing organisms. It also avoids the use of antibiotics, which could stop the growth of either the targeted Saccharibacteria species or their hosts. Using the method demonstrated here, we have successfully cultured 32 isolates from the Saccharibacteria phylum.

<table><tbody><tr><td>Agarose</td><td>Fisher Scientific</td><td>BP160-100</td><td></td></tr><tr><td>Alphaimager</td><td>Cell Biosciences</td><td>FluorChem HD2</td><td>Or equivalent UV gel imaging system</td></tr><tr><td>Aluminum foil</td><td>Fisher Scientific</td><td>01-213-101</td><td></td></tr><tr><td>Brain Heart Infusion Broth (dehydrated powder)</td><td>Becton-Dickinson</td><td>211059</td><td>Or other growth media suitable for target organisms</td></tr><tr><td>Centrifuge Rotor 70-Ti</td><td>Beckman Coulter</td><td>337922</td><td></td></tr><tr><td>Cryovials</td><td>Fisher Scientific</td><td>12-567-500</td><td></td></tr><tr><td>DMSO</td><td>Fisher Scientific</td><td>BP231-100</td><td></td></tr><tr><td>Electrophoresis Power Supply</td><td>Bio-Rad</td><td>1645052</td><td></td></tr><tr><td>Electrophoresis Rig</td><td>Bio-Rad</td><td>1704467</td><td></td></tr><tr><td>Filter Forceps</td><td>Millipore Sigma</td><td>XX6200006P</td><td>Not essential, helps ensure filters are not punctured during handling</td></tr><tr><td>Glycerol</td><td>Fisher Scientific</td><td>G33-500</td><td></td></tr><tr><td>GoTaq Green Mastermix</td><td>Promega</td><td>M7122</td><td></td></tr><tr><td>Mastercycler Pro Thermocycler</td><td>Eppendorf</td><td>950040025</td><td>Or equivalent thermocycler for PCR</td></tr><tr><td>MgCl2 solution 25mM</td><td>Promega</td><td>A3513</td><td></td></tr><tr><td>Molecular Biology grade water</td><td>Fisher Scientific</td><td>BP2819100</td><td></td></tr><tr><td>O2 Control InVitro Glove Box</td><td>Coy Laoratories</td><td>031615</td><td>If needed for microaerobic organisms</td></tr><tr><td>Optima L-100 XP High Speed Centrifuge</td><td>Beckman Coulter</td><td>8043-30-1124</td><td></td></tr><tr><td>P-10 micro pipette</td><td>Gilson</td><td>F144802</td><td></td></tr><tr><td>P-1000 micro pipette</td><td>Gilson</td><td>F123601G</td><td></td></tr><tr><td>P-2 micro pipette</td><td>Gilson</td><td>F144801</td><td></td></tr><tr><td>P-20 micro pipette</td><td>Gilson</td><td>F123600</td><td></td></tr><tr><td>P-200 micro pipette</td><td>Gilson</td><td>F123602G</td><td></td></tr><tr><td>PBS</td><td>Fisher Scientific</td><td>BP399500</td><td></td></tr><tr><td>PCR tubes 0.2 mL</td><td>Fisher Scientific</td><td>14-230-205</td><td></td></tr><tr><td>Peptone</td><td>Fisher Scientific</td><td>BP1420-500</td><td></td></tr><tr><td>Pipette tips - 10 &amp;mu;L</td><td>Fisher Scientific</td><td>02-717-157</td><td></td></tr><tr><td>Pipette tips - 1000 &amp;mu;L</td><td>Fisher Scientific</td><td>02-717-166</td><td></td></tr><tr><td>Pipette tips - 20 &amp;mu;L</td><td>Fisher Scientific</td><td>02-717-161</td><td></td></tr><tr><td>Pipette tips - 200 &amp;mu;L</td><td>Fisher Scientific</td><td>02-717-165</td><td></td></tr><tr><td>Polycarbonate filters - 47mm, 0.2 &amp;mu;m pore size</td><td>Millipore</td><td>GTTP04700</td><td></td></tr><tr><td>Screw-cap conical centrifuge tubes 15 mL</td><td>Falcon</td><td>352096</td><td>Or other tube suitable for bacterial culture</td></tr><tr><td>Sodium chloride</td><td>Fisher Scientific</td><td>BP358-1</td><td></td></tr><tr><td>Swin-Lok Filter&amp;nbsp; - 47mm</td><td>Whatman</td><td>4200400</td><td></td></tr><tr><td>SYBR Safe DNA Gel stain</td><td>ThermoFisher Scientific</td><td>S33102</td><td></td></tr><tr><td>Syringes - 20 mL</td><td>Fisher Scientific</td><td>14-955-460</td><td></td></tr><tr><td>TAE Buffer (50x) concentrate</td><td>Fisher Scientific</td><td>P1332500</td><td></td></tr><tr><td>Thickwall Polycarbonate 25 x 89 mm (26.3mL capacity) centrifuge tubes with caps</td><td>Beckman Coulter</td><td>355618</td><td></td></tr><tr><td>Tryptic Soy Blood Agar Plates</td><td>Northeast Laboratory Services</td><td>P1100</td><td>Or other agar plate sufficient for growth of host organisms</td></tr><tr><td>Tryptic Soy Broth (dehydrated powder)</td><td>Becton-Dickinson</td><td>211825</td><td>Or other growth media suitable for target organisms</td></tr><tr><td>Vinyl Anaerobic Chamber</td><td>Coy Laboratories</td><td>032714</td><td>If needed for anaerobic organisms</td></tr><tr><td>Vortex mixer</td><td>Scientific Industries</td><td>SI-0236</td><td></td></tr><tr><td>Yeast Extract</td><td>Fisher Scientific</td><td>BP1422-500</td><td></td></tr></tbody></table>

establishing stable binary cultures of symbiotic saccharibacteria from the oral cavity

Many bacterial species cannot be cultured in the laboratory using standard methods, posing a significant barrier to studying the majority of microbial diversity on earth. Novel approaches are required to culture these uncultured bacteria so that investigators can effectively study their physiology and lifestyle using the powerful tools available in the laboratory. The Candidate Phyla Radiation (CPR) is one of the largest groups of uncultivated bacteria, comprising ~15% of the living diversity on earth. The first isolate of this group was a member of the Saccharibacteria phylum, 'Nanosynbacter lyticus' strain TM7x. TM7x is an unusually small bacterium that lives as a symbiont in direct contact with a bacterial host, Schaalia odontolytica, strain XH001. Taking advantage of the unusually small cell size and its lifestyle as a symbiotic organism, we developed a protocol to rapidly culture Saccharibacteria from dental plaque. This protocol will show how to filter a suspension of dental plaque through a 0.2 &#181;m filter, then concentrate the collected Saccharibacteria cells and infect a culture of host organisms. The resulting coculture can be passaged as any normal bacterial culture and infection is confirmed by PCR. The resulting binary culture can be maintained in the laboratory and used for future experiments. While contamination is a possibility, the binary culture can be purified by either further filtering and reinfection of host, or by plating the binary culture and screening for infected colonies. We hope this protocol can be expanded to other sample types and environments, leading to the cultivation of many more species in the CPR.

PCR for detection of Saccharibacteria may appear negative (i.e., no product seen) in initial infection cultures due to a low number of Saccharibacteria symbionts. However, after a few passages a strong PCR product should appear showing that a stable infection has occurred (Figure 1A). Conversely, some infections will initially appear positive by PCR, but diminish to undetectable after 1-4 passages (not shown). This indicates that a large amount of Saccharibacteria cells were present in the initial filtrate but were diluted out by passage and none were able to enter into a stable symbiosis with the host culture. Testing several host species with the same Saccharibacteria filtrate from the oral cavity will usually have a low success rate (Figure 1B) as the symbiont-host interaction is very specific. A researcher may also test the same host with filtrates from several different subjects. If a good host organism (such as Arachnia propionica or Schaalia odontolytica) is used, a success rate of 50% can be expected.
Testing by PCR is crucial. Experienced researchers have attempted to confirm infection by microscopy, only to report false positives. The Saccharibacteria cells are small and difficult to distinguish between vesicles or irregular cell envelope bulges. A PCR signal stable through several passages is key to confirm a successful infection.
As the infected cultures grow, normal turbid growth should appear. As the symbiosis establishes itself, infected cultures will appear less turbid than cultures of uninfected host organisms (Figure 2A). In some cases, infected cultures may appear to stop growing completely and not become turbid at all. This may be due to an infection where the Saccharibacteria cells are overwhelming the host organism. Adding &#34;fresh&#34; (uninfected) host to these cultures should provide a sufficient population of host to support the continued growth of the Saccharibacteria parasites.
Overgrowth, or excessively turbid cultures, may indicate contamination by either a laboratory contaminant or another small oral bacterium that was able to pass through the 0.2 &#181;m filter. Campylobacter and Capnocytophaga spp. are typical oral contaminants of these experiments. This can be confirmed by plating the culture and looking for colonies that are atypical of the host organism followed by 16S rRNA sequencing. If contamination is seen, filtering these cultures through a 0.2 &#181;m filter is usually sufficient to remove the contaminants. Saccharibacteria cells in the filtrate can be concentrated by centrifugation and used to re-infect a pure host culture.
Another way to purify a contaminated culture is by picking infected colonies from plating an infected culture. Colonies of infected hosts can sometimes be identified by irregular colony shape compared to uninfected colonies (Figure 2B-D). These irregular colonies are dependent on the titer of Saccharibacteria in the binary culture and a smaller proportion of colonies will appear irregular if the titer is low. This can make it easy to identify infected colonies, which can be picked and used to start a pure binary culture. If no irregular colonies are seen on plating from a Saccharibacteria infected culture, it is possible that the symbiont is at a low titer or does not cause irregularly shaped colonies. In such a case, PCR screening colonies with a normal appearance can show infection by Saccharibacteria, but at a low rate (2-10% of all colonies).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/62484/62484fig1v2.jpg" /> 
Figure 1: Typical PCR results of Saccharibacteria infections of host cultures. (A) A PCR product indicating presence of Saccharibacteria may not appear with the initial infection but can appear and become stronger in subsequent passages as the coculture establishes itself. (B) Most hosts infected with Saccharibacteria-enriched filtrate will not support their growth due to the specificity of the symbiosis. In this example, only A. propionica was successfully infected. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/62484/62484fig1v2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/62484/62484fig02.jpg" /> 
Figure 2: Growth characteristics of Saccharibacteria infected cultures. (A) Growth curves of infected and uninfected cultures of A. propionica showing infected culture will not grow to the same density as the uninfected control and appear less turbid. (B-D) Plating of cocultures can produce irregular colonies, caused by Saccharibateria infections. Irregular colonies will decrease in proportion relative to the titer of Saccharibacteria in the coculture. (B) Host with a high level of Saccharibacteria. (C) 10-fold diluted Saccharibacteria (D) Uninfected host culture. White arrows indicate examples of irregular colonies. Scale bar= 1 cm.&#160;<a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/62484/62484fig02large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Establishing Stable Binary Cultures of Symbiotic Saccharibacteria from the Oral Cavity at JoVE.com

Establishing Stable Binary Cultures of Symbiotic Saccharibacteria from the Oral Cavity

We demonstrate a method for isolating difficult-to-grow members of the novel bacterial phylum, Saccharibacteria, by filtering dental plaque and co-culturing with host bacteria.

Many bacterial species cannot be cultured in the laboratory using standard methods, posing a significant barrier to studying the majority of microbial ...

establishing-stable-binary-cultures-symbiotic-saccharibacteria-from

Nanyang Technological University

Research

JoVE Journal

Biology

3.1K Views.  The Forsyth Institute. Saccharibacteriën zijn obligate parasieten die co-kweek met geschikte gastheerbacteriën vereisen. Omdat menselijke orale saccharibacteriën gemakkelijk kunnen worden geïsoleerd voor de meeste individuen met behulp van bekende gastheerbacteriële soorten. Dit protocol stelt elke onderzoeker of laboratorium in staat om zijn eigen stammen te isoleren in binaire co-cultuur.Deze techniek maakt gebruik van eenvoudige apparaten en apparatuur die aanwezig zijn in de meeste microbiologische ...

Video: Establishing Stable Binary Cultures of Symbiotic Saccharibacteria from the Oral Cavity

Oral Biofilm Analysis of Palatal Expanders by Fluorescence In-Situ Hybridization and Confocal Laser Scanning Microscopy

Confocal laser scanning microscopy (CLSM) of natural heterogeneous biofilm is today facilitated by a comprehensive range of staining techniques, one of them being fluorescence in situ hybridization (FISH).1,2 We performed a pilot study in which oral biofilm samples collected from fixed orthodontic appliances (palatal expanders) were stained by FISH, the objective being to assess the three-dimensional organization of natural biofilm and plaque accumulation.3,4 FISH creates an opportunity to stain cells in their native biofilm environment by the use of fluorescently labeled 16S rRNA-targeting probes.4-7,19 Compared to alternative techniques like immunofluorescent labeling, this is an inexpensive, precise and straightforward labeling technique to investigate different bacterial groups in mixed biofilm consortia.18,20 General probes were used that bind to Eubacteria (EUB338 + EUB338II + EUB338III; hereafter EUBmix),8-10 Firmicutes (LGC354 A-C; hereafter LGCmix),9,10 and Bacteroidetes (Bac303).11 In addition, specific probes binding to Streptococcus mutans (MUT590)12,13 and Porphyromonas gingivalis (POGI)13,14 were used. The extreme hardness of the surface materials involved (stainless steel and acrylic resin) compelled us to find new ways of preparing the biofilm. As these surface materials could not be readily cut with a cryotome, various sampling methods were explored to obtain intact oral biofilm. The most workable of these approaches is presented in this communication. Small flakes of the biofilm-carrying acrylic resin were scraped off with a sterile scalpel, taking care not to damage the biofilm structure. Forceps were used to collect biofilm from the steel surfaces. Once collected, the samples were fixed and placed directly on polysine coated glass slides. FISH was performed directly on these slides with the probes mentioned above. Various FISH protocols were combined and modified to create a new protocol that was easy to handle.5,10,14,15 Subsequently the samples were analyzed by confocal laser scanning microscopy. Well-known configurations3,4,16,17 could be visualized, including mushroom-style formations and clusters of coccoid bacteria pervaded by channels. In addition, the bacterial composition of these typical biofilm structures were analyzed and 2D and 3D images created.

We present a protocol for structural and compositional analysis of natural oral biofilm from orthodontic appliances with in situ hybridization (FISH) and confocal laser scanning microscopy (CLSM). Oral biofilm samples were collected from palatal expanders, scraping acrylic-resin flakes off their surface and referring them for molecular processing.

Confocal laser scanning microscopy (CLSM) of natural heterogeneous biofilm is today facilitated by a comprehensive range of staining techniques, one of ...

Medicine

Assessing the Viability of a Synthetic Bacterial Consortium on the In Vitro Gut Host-microbe Interface

The interplay between host and microbiota has been long recognized and extensively described. The mouth is similar to other sections of the gastrointestinal tract, as resident microbiota occurs and prevents colonisation by exogenous bacteria. Indeed, more than 600 species of bacteria are found in the oral cavity, and a single individual may carry around 100 different at any time. Oral bacteria possess the ability to adhere to the various niches in the oral ecosystem, thus becoming integrated within the resident microbial communities, and favouring growth and survival. However, the flow of bacteria into the gut during swallowing has been proposed to disturb the balance of the gut microbiota. In fact, oral administration of P. gingivalis shifted bacterial composition in the ileal microflora. We used a synthetic community as a simplified representation of the natural oral ecosystem, to elucidate the survival and viability of oral bacteria subjected to simulated gastrointestinal transit conditions. Fourteen species were selected, subjected to in vitro salivary, gastric, and intestinal digestion processes, and presented to a multicompartment cell model containing Caco-2 and HT29-MTX cells to simulate the gut mucosal epithelium. This model served to unravel the impact of swallowed bacteria on cells involved in the enterohepatic circulation. Using synthetic communities allows for controllability and reproducibility. Thus, this methodology can be adapted to assess pathogen viability and subsequent inflammation-associated changes, colonization capacity of probiotic mixtures, and ultimately, potential bacterial impact on the presystemic circulation.

Assessing the Viability of a Synthetic Bacterial Consortium on the In Vitro Gut Host-microbe Interface

Gut host-microbe interactions were assessed using a novel approach combining a synthetic oral community, in vitro gastrointestinal digestion, and a model of the small intestine epithelium. We present a method that can be adapted to evaluate cell invasion of pathogens and multi-species biofilms, or even to test probiotic formulations&#39; survivability.

The interplay between host and microbiota has been long recognized and extensively described. The mouth is similar to other sections of the ...

Biochemistry

Porphyromonas gingivalis as a Model Organism for Assessing Interaction of Anaerobic Bacteria with Host Cells

Anaerobic bacteria far outnumber aerobes in many human niches such as the gut, mouth, and vagina. Furthermore, anaerobic infections are common and frequently of indigenous origin. The ability of some anaerobic pathogens to invade human cells gives them adaptive measures to escape innate immunity as well as to modulate host cell behavior. However, ensuring that the anaerobic bacteria are live during experimental investigation of the events may pose challenges. Porphyromonas gingivalis, a Gram-negative anaerobe, is capable of invading a variety of eukaryotic non-phagocytic cells. This article outlines how to successfully culture and assess the ability of P. gingivalis to invade human umbilical vein endothelial cells (HUVECs). Two protocols were developed: one to measure bacteria that can successfully invade and survive within the host, and the other to visualize bacteria interacting with host cells. These techniques necessitate the use of an anaerobic chamber to supply P. gingivalis with an anaerobic environment for optimal growth.
The first protocol is based on the antibiotic protection assay, which is largely used to study the invasion of host cells by bacteria. However, the antibiotic protection assay is limited; only intracellular bacteria that are culturable following antibiotic treatment and host cell lysis are measured. To assess all bacteria interacting with host cells, both live and dead, we developed a protocol that uses fluorescent microscopy to examine host-pathogen interaction. Bacteria are fluorescently labeled with 2&#39;,7&#39;-Bis-(2-carboxyethyl)-5-(and-6)-carboxyfluorescein acetoxymethyl ester (BCECF-AM) and used to infect eukaryotic cells under anaerobic conditions. Following fixing with paraformaldehyde and permeabilization with 0.2% Triton X-100, host cells are labeled with TRITC phalloidin and DAPI to label the cell cytoskeleton and nucleus, respectively. Multiple images taken at different focal points (Z-stack) are obtained for temporal-spatial visualization of bacteria. Methods used in this study can be applied to any cultivable anaerobe and any eukaryotic cell type.

Porphyromonas gingivalis as a Model Organism for Assessing Interaction of Anaerobic Bacteria with Host Cells

This article presents two protocols: one to measure anaerobic bacteria that can successfully invade and survive within the host, and the other to visualize anaerobic bacteria interacting with host cells. This study can be applied to any cultivable anaerobe and any eukaryotic cell type.

Anaerobic bacteria far outnumber aerobes in many human niches such as the gut, mouth, and vagina. Furthermore, anaerobic infections are common and ...

Immunology and Infection

Determination of Biofilm Initiation on Virus-infected Cells by Bacteria and Fungi

The study of polymicrobial interactions across the taxonomic kingdoms that include fungi, bacteria and virus have not been previously examined with respect to how viral members of the microbiome affect subsequent microbe interactions with these virus-infected host cells. The co-habitation of virus with bacteria and fungi is principally present on the mucosal surfaces of the oral cavity and genital tract. Mucosal cells, particularly those with persistent chronic or persistent latent viral infections, could have a significant impact on members of the microbiome through virus alteration in number and type of receptors expressed. Modification in host cell membrane architecture would result in altered ability of subsequent members of the normal flora and opportunistic pathogens to initiate the first step in biofilm formation, i.e., adherence. This study describes a method for quantitation and visual examination of HSV&#39;s effect on the initiation of biofilm formation (adherence) of S. aureus and C. albicans.

A method is described herein for the determination of inter-Kingdom association and competition (bacterial and fungal) for adherence to virus-infected HeLa cell monolayers. This protocol can be extended to multiple combinations of prokaryotes, eukaryotes, and viruses.

The study of polymicrobial interactions across the taxonomic kingdoms that include fungi, bacteria and virus have not been previously examined with ...

Using Coculture to Detect Chemically Mediated Interspecies Interactions

In nature, bacteria rarely exist in isolation; they are instead surrounded by a diverse array of other microorganisms that alter the local environment by secreting metabolites. These metabolites have the potential to modulate the physiology and differentiation of their microbial neighbors and are likely important factors in the establishment and maintenance of complex microbial communities. We have developed a fluorescence-based coculture screen to identify such chemically mediated microbial interactions. The screen involves combining a fluorescent transcriptional reporter strain with environmental microbes on solid media and allowing the colonies to grow in coculture. The fluorescent transcriptional reporter is designed so that the chosen bacterial strain fluoresces when it is expressing a particular phenotype of interest (i.e. biofilm formation, sporulation, virulence factor production, etc.) Screening is performed under growth conditions where this phenotype is not expressed (and therefore the reporter strain is typically nonfluorescent). When an environmental microbe secretes a metabolite that activates this phenotype, it diffuses through the agar and activates the fluorescent reporter construct. This allows the inducing-metabolite-producing microbe to be detected: they are the nonfluorescent colonies most proximal to the fluorescent colonies. Thus, this screen allows the identification of environmental microbes that produce diffusible metabolites that activate a particular physiological response in a reporter strain. This publication discusses how to: a) select appropriate coculture screening conditions, b) prepare the reporter and environmental microbes for screening, c) perform the coculture screen, d) isolate putative inducing organisms, and e) confirm their activity in a secondary screen. We developed this method to screen for soil organisms that activate biofilm matrix-production in Bacillus subtilis; however, we also discuss considerations for applying this approach to other genetically tractable bacteria.

Bacteria produce secreted compounds that have the potential to affect the physiology of their microbial neighbors. Here we describe a coculture screen that allows detection of such chemically mediated interspecies interactions by mixing soil microbes with fluorescent transcriptional reporter strains of Bacillus subtilis on solid media.

In nature, bacteria rarely exist in isolation; they are instead surrounded by a diverse array of other microorganisms that alter the local environment by ...

Protocol for Co-Culturing Sucrose-Secreting Cyanobacteria with Fungal Partners

Assembly and Quantification of Co-Cultures Combining Heterotrophic Yeast with Phototrophic Sugar-Secreting Cyanobacteria

With the increasing demand for sustainable biotechnologies, mixed consortia containing a phototrophic microbe and heterotrophic partner species are being explored as a method for solar-driven bioproduction. One approach involves the use of CO2-fixing cyanobacteria that secrete organic carbon to support the metabolism of a co-cultivated heterotroph, which in turn transforms the carbon into higher-value goods or services. In this protocol, a technical description to assist the experimentalist in the establishment of a co-culture combining a sucrose-secreting cyanobacterial strain with a fungal partner(s), as represented by model yeast species, is provided. The protocol describes the key prerequisites for co-culture establishment: Defining the media composition, monitoring the growth characteristics of individual partners, and the analysis of mixed cultures with multiple species combined in the same growth vessel. Basic laboratory techniques for co-culture monitoring, including microscopy, cell counter, and single-cell flow cytometry, are summarized, and examples of nonproprietary software to use for data analysis of raw flow cytometry standard (FCS) files in line with FAIR (Findable, Accessible, Interoperable, Reusable) principles are provided. Finally, commentary on the bottlenecks and pitfalls frequently encountered when attempting to establish a co-culture with sugar-secreting cyanobacteria and a novel heterotrophic partner is included. This protocol provides a resource for researchers attempting to establish a new pair of co-cultured microbes that includes a cyanobacterium and a heterotrophic microbe.

This protocol provides a comprehensive guideline for the setup and quantitative monitoring of co-cultures, including photoautotrophic sugar-secreting cyanobacteria and heterotrophic yeasts.

With the increasing demand for sustainable biotechnologies, mixed consortia containing a phototrophic microbe and heterotrophic partner species are being ...

Bioengineering

Organotypic Tissue Model Systems for Investigating Host-Pathogen Interactions In Vitro

Recapitulating the host-pathogen interface at the epithelial or mucosal barrier in vitro remains a challenging prospect for infection biologists. While in-house grown 2D epithelial monolayers lack true representation of the in vivo situation, commercially available tissue models are often overlooked due to their cost and practicality. However, with careful planning, such models provide reproducible platforms for a vast array of different applications. Here, we report the use of epithelial models that can be utilized for a wide variety of experimental purposes to investigate host-pathogen interactions in various ecological niches, such as the oral cavity, skin, and vaginal mucosa. From simple planktonic cells to complex biofilm co-culture, epithelial models are used to assess microbial adherence and invasion, and to evaluate the host response at a transcriptional and/or protein level, with scope for more detailed profiling using different omics approaches. Furthermore, these biological systems can be used as more accurate test beds for evaluating conventional and novel antimicrobial activity in a complex host-pathogen microenvironment in vitro. The protocols described herein document how models are handled upon arrival and prepared in the laboratory for co-culture stimulation with biofilm communities. The methods detail how experimental outputs are achieved from the model systems, including the processing of tissue, the co-culture setup, and data generation. These experiments include host gene expression through single- and multiplex qPCR analyses and inflammatory protein detection using ELISAs. In conclusion, epithelial models provide useful in vitro systems for preclinical investigatory studies into simple or complex host-pathogen interactions.

The present protocol outlines the application of organotypic tissue models for investigating host-pathogen interactions in vitro. Specifically, the model system described uses a multi-layered oral epithelium exposed to microorganisms associated with biofilms (dental plaque) within the context of oral health versus disease.

Recapitulating the host-pathogen interface at the epithelial or mucosal barrier in vitro remains a challenging prospect for infection biologists. While ...

Diagnosis and Strain Identification of pSS-Related Oral Candida

Examination of Oral Candida Infection in Primary Sj&#246;gren&#39;s Syndrome Patients

Primary Sj&#246;gren's syndrome (pSS) is an autoimmune disease characterized by symptoms such as dry mouth, dry eyes, and other systematic symptoms. Due to the hyposalivation experienced by pSS patients, oral dysbacteriosis often occurs. A common complication of pSS is the oral Candida infection. In this article, the authors describe systematic methods that can effectively diagnose oral Candida infection and identify the Candida strains using saliva, oral mucosal swabs, or mouthwash from pSS patients. The Sabouraud's Dextrose Agar (SDA), hyphal formation assay, potassium hydroxide (KOH) smear test, and calcofluor white (CFW) staining assay are used for the diagnosis of oral Candida infection. A Candida diagnostic agar is used for the identification of Candida strains. Finally, antifungal susceptibility testing is used to determine appropriate antifungal drug treatment. This standardized method can enhance the diagnosis, treatment, and future research of pSS-related oral Candida infections. Early diagnosis, using this method, can also prevent any complications arising due to delay in receiving appropriate treatment.

Author Spotlight: Oral Candida Diagnosis to Advance Clinical Treatment Regimen for pSS Patients

Here, we present a protocol for the examination of oral Candida infection in patients with primary Sj&#246;gren's syndrome, which can be used for timely treatment and, thereafter, avoiding related complications.

Primary Sj&#246;gren's syndrome (pSS) is an autoimmune disease characterized by symptoms such as dry mouth, dry eyes, and other systematic symptoms. Due ...

Measuring the Migration and Biofilm Formation of Various Bacteria

As microbes that thrive in the host body primarily have adaptive abilities that facilitate their survival, methods for classifying and identifying their nature would be beneficial in facilitating their characterization. Currently, most studies focus only on one specific characterization method; however, the isolation and identification of microorganisms from the host is a continuous process and usually requires several combinatorial characterization methods. Herein, we describe methods of identifying the microbial biofilm-forming ability, the microbial respiration state, and their chemotaxis behavior. The methods are used to identify five microbes, three of which were isolated from the bone tissue of Sprague-Dawley (SD) rats (Corynebacterium stationis, Staphylococcus cohnii subsp. urealyticus, and Enterococcus faecalis) and two from the American Type Culture Collection (ATCC)-Staphylococcus aureus ATCC 25923&#160;and Enterococcus faecalis V583. The microbes isolated from the SD rat bone tissue include the gram-positive microbes. These microbes have adapted to thrive under stressful and nutrient-limiting environments within the bone matrix. This article aims to provide the readers with the specific know-how of determining the nature and behavior of the isolated microbes within a laboratory setting.

Here, we present a practical method for the isolation and identification of microorganisms within the host. In this way, the physicochemical properties of microorganisms and possible ways of living in the host are clearly described.

As microbes that thrive in the host body primarily have adaptive abilities that facilitate their survival, methods for classifying and identifying their ...

In Vitro Polymicrobial Interactions in Cystic Fibrosis Lung Infections

Growing a Cystic Fibrosis-Relevant Polymicrobial Biofilm to Probe Community Phenotypes

Most in vitro models lack the capacity to fully probe bacterial phenotypes emerging from the complex interactions observed in real-life environments. This is particularly true in the context of hard-to-treat, chronic, and polymicrobial biofilm-based infections detected in the airways of individuals living with cystic fibrosis (CF), a multiorgan genetic disease. While multiple microbiome studies have defined the microbial compositions detected in the airway of people with CF (pwCF), no in vitro models thus far have fully integrated critical CF-relevant lung features. Therefore, a significant knowledge gap exists in the capacity to investigate the mechanisms driving the pathogenesis of mixed species CF lung infections. Here, we describe a recently developed four-species microbial community model, including Pseudomonas aeruginosa, Staphylococcus aureus, Streptococcus sanguinis, and Prevotella melaninogenica grown in CF-like conditions. Through the utilization of this system, clinically relevant phenotypes such as antimicrobial&#160;recalcitrance of several pathogens were observed and explored at the molecular level. The usefulness of this in vitro model resides in its standardized workflow that can facilitate the study of interspecies interactions in the context of chronic CF lung infections.

This protocol describes a cystic fibrosis (CF) lung-relevant four-species polymicrobial biofilm model that can be used to explore the impact of bacterial interspecies interactions.

Most in vitro models lack the capacity to fully probe bacterial phenotypes emerging from the complex interactions observed in real-life environments. This ...

Establishing Stable Binary Cultures of Symbiotic Saccharibacteria from the Oral Cavity

Samenvatting

Meer video's verkennen