This work was supported by the National Institute of Health (1 R01 GM095384-01) awarded to Forest Rohwer. We thank Epicentre, an Illumina company for providing early access to Ribo-Zero Epidemiology kits. We thank Mark Hatay for the design and production of the ultracentrifugation tube holder. We thank Andreas Haas and Benjamin Knowles for critical readings and discussions of the manuscript, and Lauren Paul for assisting the filming process.

NOTE: Induced sputum samples were collected in accordance with the University of California Institutional Review Board (HRPP 081500) and San Diego State University Institutional Review Board (SDSU IRB#2121), by the research coordinator of the University of California, San Diego (UCSD) adult CF clinic.
1. Sample Collection and Pre-treatment (Pre-treat Samples within 30 Min After Collection)
<ol>
	<li>Prior to sample collection, label four 15 ml tubes as: (i) viral metagenome, (ii) microbial metagenome, (iii) metatranscriptome, and (iv) extra sputum. Repeat for each sample. Add 2 ml of 0.1 mm silica beads into the tube labeled &#8220;Metatranscriptome&#8221;, followed by 6 ml of guanidine isothiocyanate-based RNA lysis buffer (GITC-lysis buffer).</li>
	<li>During sample collection, use sterile saline solution (60 ml) as a mouth rinse to minimize contamination by oral microbes. Collect sputum samples over a 30 min time period after the inhalation of 4 ml of 7% hypertonic saline via a nebulizer. Process samples immediately, as described below.</li>
	<li>Dilute the sample to a total volume of 8 ml.
	<ol>
		<li>Estimate sample volume by weighing empty sputum cup before and after sample collection.</li>
		<li>If the volume of sample is less than 8 ml, add appropriate amount of 0.02 &#956;m-filtered 1x PBS to generate a total sample volume of at least 8 ml.</li>
		<li>Immediately homogenize the sample with a 3 ml syringe until no visible clumps remain within the sputum</li>
		<li>Using the same syringe, draw up 2 ml of sputum and proceed immediately to step 1.4.</li>
	</ol>
	</li>
	<li>Preserving Total RNA from Sputum Sample
	<ol>
		<li>Inject 2 ml sputum sample from step 1.3.4 into the &#8220;metatranscriptome&#8221; tube containing silica beads and GITC-lysis buffer.</li>
		<li>Close the lid and seal the tube securely with Parafilm to avoid leakage.</li>
		<li>Homogenize the sputum immediately at medium speed for 10 min. Depending on the vortexer available, place the tube horizontally and secure with tape if necessary.</li>
		<li>Keep the tube at 4 &#176;C or in an ice box and transport to the laboratory if necessary.</li>
	</ol>
	</li>
	<li>Using the same syringe, aliquot 2 ml of sputum each into the tubes labeled &#8220;viral metagenome&#8221; and &#8220;microbial metagenome&#8221; and transfer the remaining sputum from the sputum cup into the tube labeled &#8220;extra sputum&#8221;.</li>
	<li>Store all tubes at 4 &#176;C or ice box and transport to the laboratory if necessary.</li>
</ol>
2. Generating Viral Metagenome
<ol>
	<li>Preparation of Buffers and Solutions
	<ol>
		<li>Prepare 50 mM dithiothreitol (DTT) in advance and store at 4 &#176;C. This is stable for 2 weeks.</li>
		<li>Prepare Saline Magnesium (SM) buffer (250 ml): 1 M NaCl, 10 mM MgSO4, 50 mM Tris-HCl; adjust pH to 7.4. Filter sterilize (0.02 &#181;m pore size) and store at room temperature.</li>
		<li>Prepare DNase I enzyme to 100 U/&#181;l (in molecular grade water) from lyophilized bovine pancreas DNase I according to the activity defined by Dornase unit/mg dry weight.</li>
		<li>Prepare 10x DNase I buffer (50 ml): 100 mM MgCl2, 20 mM CaCl2; adjust pH to 6.5. Filter sterilize (0.02 &#181;m pore size) and store at room temperature.</li>
		<li>Prepare 4% paraformaldehyde.</li>
		<li>Prepare 200x TE Buffer: 2 M Tris-HCl (pH 8.5), 0.2 M EDTA. Filter sterilize (0.02 &#181;m pore size) and store at room temperature.</li>
		<li>Prepare 10 ml of 10% Sodium Dodecyl Sulfate (SDS) using molecular grade water.</li>
		<li>Prepare 50 ml CTAB/NaCl (10% CTAB. 700 mM NaCl) using molecular grade water. Dissolve CTAB overnight. If precipitates persist, heat up the solution at 65 &#176;C. Solution is highly viscous in room temperature. 
		NOTE: The filtration of buffers using 0.02 &#956;m filter allows the removal of viral-like particles within the solution, but not free nucleic acid contamination.</li>
	</ol>
	</li>
	<li>Sample Pre-treatment
	<ol>
		<li>Prepare appropriate amount of fresh 6.5 mM dithiothreitol (DTT).</li>
		<li>Dilute the homogenate by adding 0.02 &#181;m-filtered SM buffer to generate a total volume of 6 ml.</li>
		<li>To aid in mucus dissolution, add equal volume (6 ml) of 6.5 mM dithiothreitol (DTT) to the sample, vortex vigorously to mix and incubate for 1 hr at 37 &#176;C.</li>
		<li>Vortex the treated sample vigorously and spin at 10 &#176;C, 3,056 x g for 15-20 min.</li>
		<li>Collect the supernatant into a new 15 ml tube.</li>
		<li>Repeat step 2.2.3 and 2.2.5 for the next sample.</li>
		<li>Transfer and filter the supernatant with a 0.45 &#181;m filter mounted on a syringe into a new 15 ml tube. 
		NOTE: If the filter clogs, retrieve the samples from the syringe and omit the filtration step.</li>
		<li>Take a 100 &#181;l subsample of the 0.45 &#181;m-filtered sample, perform chloroform and DNase I treatment (see section 2.3.12-2.3.15) and add equal volume of 4% paraformaldehyde to fix the sample for epifluorescence microscopy (Figure 2A).</li>
		<li>For a &#8220;catch-all&#8221; viral particles enrichment approach (see Discussion), go to step 2.3.12 to omit viral particles selection based on cesium chloride gradient ultracentrifugation. However, this may result in chloroform-resistant bacterial contamination and higher amount of host-DNA in the viral lysate.</li>
	</ol>
	</li>
	<li>Viral-like Particles (VLPs) Enrichment and Purification
	<ol>
		<li>Prepare individual cesium chloride (CsCl) solutions by dissolving the appropriate amount of CsCl with non-filtered SM buffer to the desired density (1.7 g/ml, 1.5 g/ml, 1.35 g/ml, and 1.2 g/ml). Filter each solution through a 0.02 &#181;m filter prior to use.</li>
		<li>Set up CsCl gradient as shown in Figure 2B.</li>
		<li>Load 1 ml of 1.7 g/ml into each tube, load 1 ml of 1.5 g/ml into each tube, load 1 ml of 1.35 g/ml into each tube, load 1.2 g/ml into each tube (optional), and finally load 6-8 ml sample into the respective tube. Mark individual layers to denote the location of each fraction.</li>
		<li>Balance each opposing pair of tubes to within 1 mg.</li>
		<li>Carefully load each tube into the spin bucket. Spin all buckets even if they are empty. Load the spin bucket onto the rotor.</li>
		<li>Centrifuge at 82,844 x g at 4 &#176;C for 2 hr.</li>
		<li>Following centrifugation, carefully remove the tubes from the holder without disrupting the density gradients.</li>
		<li>Using a 3 ml syringe with an 18 G needle, pierce the tube just below the 1.5 g/ml density layer (Figure 2, red arrow) and pull ~1.5 ml into the syringe.</li>
		<li>Collect the upper fraction by slowly removing the needle and allowing the remaining fraction in the tube to drip into a new 15 ml tube through the puncture. Label this as &#8220;upper fraction waste&#8221;.</li>
		<li>Collect the 1.5 g/ml fraction (containing VLPs) from the syringe by ejecting the contents into two new microfuge tubes.</li>
		<li>Repeat step 2.3.8-2.3.10 for all samples.</li>
		<li>Add 0.2 volume of chloroform into the viral concentrate, shake vigorously, incubate at RT for 10 min, spin at max speed for 5 min, and collect the aqueous phase.</li>
		<li>Add 10x DNase buffer and DNase I (final concentration = 2.5 U/&#181;l) into the chloroform-treated viral concentrate, and incubate at 37 &#176;C for 1.5-2 hr.</li>
		<li>Inactivate the DNase activity at 65 &#176;C for 15 min.</li>
		<li>Remove 15 &#181;l of the chloroform- and DNase I-treated viral fraction into a new tube, and add 15 &#181;l 4% paraformaldehyde to fix the sample for epifluorescence microscopy.</li>
	</ol>
	</li>
	<li>DNA Extraction
	<ol>
		<li>Pool viral concentrates from each sample into a cleaned and autoclaved 50 ml Oak Ridge high-speed centrifuge tube.</li>
		<li>Add the following: 0.1 volume 200x TE buffer, 10 &#956;l 0.5 M EDTA per ml of sample, 1 volume of formamide, and 10 &#956;l glycogen. Mix well and incubate at room temperature for 30 min.</li>
		<li>Using the new volumes, add 2 volumes of room temperature 100% ethanol. Mix well and incubate at 4 &#176;C for at least 30 min.</li>
		<li>Pellet DNA by spinning the tube at 17,226 x g for 20 min, at 4 &#176;C using a SS-34 rotor.</li>
		<li>Discard the supernatant carefully by using a serological pipette. Wash the pellet twice with ice-cold 70% ethanol.</li>
		<li>Remove as much liquid as possible and allow the pellet to air-dry at room temperature for 15 min.</li>
		<li>Resuspend the DNA pellet in 567 &#956;l of 1x TE buffer (pH 8.0). 
		NOTE: Allow at least 15 min for complete resuspension at room temperature. Store the resuspended DNA overnight at 4 &#176;C until further processing.</li>
		<li>Transfer the entire 567 &#956;l of resuspended DNA solution into a new 1.5 ml microfuge tube. Add 30 &#956;l of pre-warmed 10% SDS and 3 &#956;l of proteinase K (20 &#956;g/ml), mix thoroughly and incubate for 1 hr at 56 &#176;C. Pre-warm CTAB/NaCl at 65 &#176;C.</li>
		<li>Add 100 &#956;l of 5 M NaCl and mix thoroughly. Add 80 &#956;l of pre-warmed CTAB/NaCl solution, vortex, and incubate for 10 min at 65 &#176;C.</li>
		<li>Add equal volume of chloroform, vortex to mix, and spin at 16,100 x g for 5 min.</li>
		<li>Transfer the supernatant to a new 1.5 ml microfuge tube. Add an equal volume of phenol/chloroform, vortex to mix, and spin at 16,100 x g for 5 min.</li>
		<li>Transfer the supernatant to a new 1.5 ml microfuge tube. Add an equal volume of chloroform, vortex to mix, and spin at 16,100 x g for 5 min.</li>
		<li>Transfer the supernatant to a new 1.5 ml microfuge tube. Add equal volume of isopropanol to the supernatant fraction, mix, and incubate at -20 &#176;C for at least 30 min.</li>
		<li>Pellet the DNA, spin at 16,100 x g for 15 min at 4 &#176;C. Pipette off the supernatant carefully and wash the pellet twice with ice-cold 70% ethanol.</li>
		<li>Perform a short spin and remove the remaining ethanol from the tube. Air dry the pellet for 15 min.</li>
		<li>Resuspend the DNA pellet with 50 &#956;l of elution buffer (5 mM Tris, pH 8.5). Allow the pellet to rehydrate for at least 5 min in room temperature.</li>
		<li>Quantify the DNA using a high-sensitivity fluorescence-based assay.</li>
	</ol>
	</li>
	<li>Amplification using Phi29 Polymerase (Optional)
	<ol>
		<li>Prepare 2x annealing buffer: 80 mM Tris-HCl (pH 8.0), 20 mM MgCl2.</li>
		<li>Dilute Phi29 DNA polymerase to 5 U/&#956;l.</li>
		<li>Pre-mix sample buffer, comprised of 50 &#956;l random hexamer primer (100 &#956;M), 125 &#956;l 2x annealing buffer, and 25 &#956;l water. Aliquot and store at -20 &#176;C.</li>
		<li>Pre-mix reaction buffer, comprised of 100 &#956;l Phi29 10x buffer, 40 &#956;l 10 mM dNTPs, and 560 &#956;l water. Aliquot and store at -20 &#176;C.</li>
		<li>Add 1 &#956;l template DNA into 4 &#956;l sample buffer.</li>
		<li>Incubate the mixture at 95 &#176;C for 3 min and cool on ice.</li>
		<li>Add 14 &#956;l of reaction buffer into the mixture from 2.4.4, mix by pipetting up and down.</li>
		<li>Add 1 &#956;l of Phi29 DNA polymerase, mix by pipetting up and down, and incubate at 30 &#176;C for 18 hr followed by 65 &#176;C for 10 min.</li>
		<li>Clean up the reactions using genomic DNA columns or phenol/chloroform and ethanol precipitations.</li>
	</ol>
	</li>
	<li>Epifluorescence Microscopy (Refer to Haas et al. 201428 for filtration system setup) 
	NOTE: Following isolation and purification, epifluorescence microscopy with nucleic acid dyes can be used to verify the presence and purity of viral particles in samples (Figures 2A and 2C). Free DNA in the sample can give rise to high background fluorescence. Therefore, the sample should be DNase I-treated prior to fixation and staining for micrographs.
	<ol>
		<li>Prepare mount solution (0.1% ascorbic acid, 50% glycerol). Add 100 &#956;l of 10% ascorbic acid to 4.9 ml of 1x phosphate buffered saline (PBS), mix thoroughly. Add 5 ml of 100% glycerol to the mixture, mix thoroughly and label the tube as &#8220;mount&#8221;.</li>
		<li>Filter mount using a 0.02 &#956;m alumina matrix disposable syringe filter, aliquot into microfuge tubes, and store at -20 &#176;C.</li>
		<li>Aliquot 100 &#956;l of sample into a new microfuge tube and add equal volume of 4% paraformaldehyde to fix the VLPs. Incubate the mixture at room temperature for at least 10 min.</li>
		<li>Make up the volume to 1 ml by adding 800 &#956;l of 0.02 &#956;m-filtered water. Add 1 &#956;l of SYBR Gold stain into the tube and incubate at room temperature for 10 min.</li>
		<li>Set up the filtration system by turning on the vacuum pump between -9 and -10 psi (-62.1 and -68.9 kPa).</li>
		<li>Wash the pedestal with water and place a 0.02 &#181;m alumina matrix filter with annular polypropylene support ring into the filter pedestal.</li>
		<li>Place a filter tower on top of the filter pedestal with the filter and secure with a clamp.</li>
		<li>Pipette the contents from the 1.5 ml microfuge tube into the filter tower, and allow a few minutes for sample to filter through.</li>
		<li>Label and pipette 10 &#181;l of mount reagent into a microscopic slide.</li>
		<li>Leave the vacuum on while removing the filter tower and clamp.</li>
		<li>Carefully remove the filter from the filter pedestal and blot the bottom of the filter with a Kimwipe, then place the filter directly on top of the mount on the microscopic slide.</li>
		<li>Pipette another 10 &#181;l of mount reagent onto the filter and place a coverslip over the filter.</li>
	</ol>
	</li>
</ol>
3. Generating Microbial Metagenome
<ol>
	<li>Preparation of buffers and solutions
	<ol>
		<li>Prepare 50 ml of 1x DNase buffer: 50 mM NaAc, 10 mM MgCl2, 2 mM CaCl2; adjust pH to 6.5. Filter sterilize (0.22 &#181;m) and store at room temperature.</li>
		<li>Prepare DNase I enzyme to 1000 U/&#181;l (in molecular grade water) from lyophilized bovine pancreas DNase I according to the activity defined by Dornase unit/mg dry weight.</li>
		<li>Prepare 100 ml of SE buffer: 75 mM NaCl, 25 mM EDTA; adjust pH to 7.5. Filter sterilize (0.22 &#181;m) and store at room temperature.</li>
	</ol>
	</li>
	<li>Sample Pre-treatment Prior to DNA Extraction
	<ol>
		<li>Dilute the homogenate by adding 5 volumes of 0.22 &#181;m-filtered 1x PBS. For example, add 10 ml of 1x PBS into 2 ml of sample.</li>
		<li>Add &#946;-mercaptoethanol to 2% (v/v) final concentration. Rock the mixture (in the chemical hood) at room temperature for 2 hr.</li>
		<li>Spin the sample at 10 &#176;C and 3,056 x g for 15 min, and discard supernatant.</li>
		<li>Resuspend the pellet in 10 ml of molecular grade water (or 0.22 &#181;m filtered water), and incubate at room temperature for 15 min.</li>
		<li>Repeat steps 3.2.3 and 3.2.4 once.</li>
		<li>Spin at 10 &#176;C and 3,056 x g for 15 min, and discard supernatant.</li>
		<li>Resuspend the pellet in 5 ml 1x DNase buffer and add 15 &#181;l DNase I (1,000 U/&#181;l) per ml of sample.</li>
		<li>Incubate at 37 &#176;C with repeated mixing for 2 hr.</li>
		<li>Inactivate the DNase activity at 65 &#176;C for 15 min.</li>
		<li>Spin at 10 &#176;C and 3,056 x g for 15 min, and discard supernatant. Resuspend the pellet in 10 ml SE buffer.</li>
		<li>Repeat step 3.2.10.</li>
		<li>Spin at 10 &#176;C and 3,056 x g for 15 min, and discard supernatant.</li>
		<li>Resuspend the pellet in 2 ml SE buffer, and transfer to two microfuge tubes.</li>
		<li>Pellet the cells in the microfuge tubes. Spin the tubes at 16,100 x g at room temperature for 15 min.</li>
		<li>Remove the supernatant and extract DNA from the pelleted cells using a genomic DNA extraction kit, Gram-positive variation protocol.</li>
	</ol>
	</li>
</ol>
4. Generating Metatranscriptome
<ol>
	<li>Sample Pre-treatment
	<ol>
		<li>Perform mechanical lysis of cells by bead beating in GITC-lysis buffer immediately after sample collection and homogenization. See step 1.4.</li>
		<li>Spin the mixture at 4 &#176;C and 600 x g for 5 min to pellet the silica beads.</li>
		<li>Transfer the supernatant into a new tube.</li>
		<li>Add 200 &#956;l of chloroform for every 750 &#956;l of GITC-lysis buffer used, shake vigorously by hand for 15 sec, incubate at room temperature for 10 min, and spin at 4 &#176;C and 3,056 x g for 15 min. During this 15 min spin, prepare for step 4.2.</li>
		<li>After the 15 min spin (a clear separation of aqueous phase-interphase-organic phase forms), extract the aqueous phase (without disrupting the interphase) into new RNase-free tube(s). 
		NOTE: The aqueous phase contains the RNA. Keep the tubes on ice until the next step.</li>
	</ol>
	</li>
	<li>Perform total RNA extraction and purification using commercially available column-based RNA purification kits or conventional isopropanol-based RNA precipitation.
	<ol>
		<li>Silica Column-based RNA Purification
		<ol>
			<li>Measure the total volume of the aqueous fraction obtained.</li>
			<li>Add appropriate volume of RNA-binding buffer to sample and mix well.</li>
			<li>Adjust mixture to appropriate binding condition according to manufacturer&#8217;s protocol. Mix well and do a short spin.</li>
			<li>Load the mixture into the RNA-column. For a large volume sample, use multiple loading and load each column up to 4x. Otherwise, consider using multiple columns for each sample.</li>
			<li>Wash the column appropriately according to the manufacturer&#8217;s protocol.</li>
			<li>Elute the RNA with at least 30 &#181;l of RNase-free water. Double-elution will slightly increase the yield of RNA. However, this will dilute the RNA concentration.</li>
			<li>Measure the RNA concentration and proceed directly to DNase I treatment. Use the Bioanalyzer to check the quality of the RNA (recommended).</li>
		</ol>
		</li>
		<li>RNA Precipitation
		<ol>
			<li>Add an equal volume of isopropanol (e.g., 500 &#181;l of isopropanol into 500 &#181;l of aqueous fraction) and 2 &#181;l of 10 &#181;g/&#181;l RNase-free glycogen to the sample.</li>
			<li>Incubate the mixture at room temperature for 10 min.</li>
			<li>Spin at 12,000 x g and 4 &#176;C for 15 min.</li>
			<li>Carefully remove the supernatant, add 1 ml of RNase-free 75% ethanol. Spin the mixture at 7,500 x g and 4 &#176;C for 5 min to make sure the pellet is intact.</li>
			<li>Carefully remove the ethanol.</li>
			<li>Repeat steps 4.2.2.4 and 4.2.2.5 once.</li>
			<li>Air dry the pellet for 10 min.</li>
			<li>Rehydrate the pellet in 50 &#181;l of RNase-free water, incubate at 55 &#176;C for 5 min and proceed directly to DNase treatment. Use the Bioanalyzer to check the quality of the RNA (Recommended).</li>
			<li>Store RNA in aliquots at -20 &#176;C, or -80 &#176;C for long-term storage.</li>
		</ol>
		</li>
	</ol>
	</li>
</ol>

The authors have nothing to disclose.

Viral Metagenomics
Viral particles are concentrated using polyethylene glycol (PEG) precipitation or small volume concentrators. In some cases, concentration may not be needed, but pre-filtration or low speed centrifugation steps are used to remove eukaryotic and microbial cells. Viral lysates will be further enriched and purified using density gradient ultracentrifugation9,41 or small size filters (e.g., 0.45 &#956;m) to remove eukaryotic and large microbial cells25. Density gradient ultracentrifugation is typically performed with dense but inert solutions such as sucrose or cesium chloride to isolate and concentrate viral particles41. Physical separation is based on the size and buoyant density of viral particles. Therefore, proper choice of filter pore size and the rigorous preparation of gradients are essential to isolate specific viral communities, as the success of the physical recovery of VLPs determines the community isolated41 (i.e., viral particles that do not pass through the filter or fall within the extraction density will not be detected in the metagenome). After viral isolation and concentration, there may be contaminating non-viral genomic material present in the sample both in the form of free nucleic acids and microbial and eukaryotic cells. Therefore, it is critical to verify the purity of viral particles in samples (Figures 1A and&#160;1B). A chloroform treatment is commonly used to lyse remaining cells, followed by nuclease treatment to degrade free nucleic acids prior to nucleic acid extraction.
A caveat to the presented workflow was the use of density gradient separation to isolate viral particles as it may exclude enveloped viral particles that may be too buoyant to enter the CsCl gradient. An alternative &#8220;catch-all&#8221; method is to omit the density gradient separation and isolate the community DNA from the 0.45 &#956;m &#8211; filtrates treated with chloroform and DNase I. This approach is also appropriate to accommodate small sample volumes such as those from swabs or blood plasma. However, this may result in chloroform-resistant bacterial contamination and higher amount of DNase I-resistant extracellular DNA.
Current sequencing protocols require 1 ng to 1 &#956;g of nucleic acids for sequencing library preparation whereby higher DNA yields provide a wider choice of sequencing options. The DNA concentration of generated viromes often ranges from below the detection limit to more than 200 ng/&#956;l. The amount of viral nucleic acids recovered may be insufficient for direct sequencing library preparation. In such cases, nucleic acid amplification is essential. Linker amplification shotgun libraries (LASLs)2,42,43 and whole genome amplification based on multiple displacement amplification (MDA) are the two methods most commonly used to generate sufficient DNA for sequencing. MDA methods such as those based on Phi29 DNA polymerase are known to suffer from amplification biases, and may preferentially amplify ssDNA and circular DNA, resulting in non-quantitative taxonomical and functional characterization44,45. An optimized version of the LASLs approach has been shown to introduce only minimal biases, promotes higher sensitivity (for small amounts of starting material), and is easily adapted for different sequencing platforms43. However, the approach has many steps, requires specialized equipment to minimize DNA loss, and is limited to dsDNA templates. In our laboratory, this approach has been successfully adapted to amplify detectable and undetectable amount of DNA extracted from bronchoalveolar lavage-, coral- and sea water-derived VLPs (unpublished and Hurwitz&#160;et al.46).
Developing data analysis pipelines has classically been one of the most challenging aspects of viral metagenomics analysis due to the highly diverse and largely unknown nature of the viral communities. While there are an estimated 108 viral genotypes in the biosphere, to date current viral databases contain ~ 4,000 viral genomes, which is about 1/100,000th of this approximate total viral diversity. Therefore, similarity-based searches (such as BLAST47) for taxonomic and functional assignment in viral metagenomes possess inherent challenges. Many sequences fail to have significant similarities to genomes in the database, and therefore, are classified as unknown. Even though homology-based searches are the most important applications for assigning taxonomy and function to sequence data, alternative approaches based on database-independent analysis have been developed48-50. Fancello et al.51 provide a complete review of computational tools and algorithms used in viral metagenomics.
Microbial Metagenomics
Typically, the total amount of DNA extracted from hypotonic lysis-treated microbial communities (HL-DNA) range from 20 ng to 5 &#956;g. The yield is highly dependent on the patient&#8217;s health status and the amount of sputum sample collected, which explains the variations seen in the total yield of HL-DNA extracted in this study (Table 2). The critical steps to generate good quality sequence data rely on the quality of sequencing libraries generated. Figure 2 shows a typical size range for the sequencing libraries generated from CF sputum-derived microbial DNA using an enzymatic-based DNA fragmentation procedure. The optimal library size is dependent on the choice of sequencing platform and application, and therefore, the fragmentation procedure can be optimized, if necessary, through alternative approaches such as sonication and nebulization. In addition to the presented representative results, the success of the presented method on CF sputum collected from multiple patients across multiple time points is also illustrated in Lim et al. (2012)9 and Lim et al. (2014)10.
Previous studies9,10 suggest that every patient harbors a unique set of microbial community that shifts over time, thereby reflecting the persistence of the major players within the community while fluctuations are likely due to perturbations such as antibiotic treatments. Whether these fluctuations occur daily even without external perturbations or due to sampling procedure and sample processing, is still in question. Based on the HL-DNA metagenomic and 16S rDNA amplicon analysis, the 7-day longitudinal sampling shows that the daily fluctuation of microbial profiles without antibiotic perturbation (Day 1, 2, and 3) was minimal (Figures 3A and&#160;3B). Upon introduction of oral antibiotics immediately after the Day 3 sampling, changes in the community profile became apparent on Day 4. While the antibiotic ciprofloxacin targets a broad spectrum of known bacterial pathogens such as P. aeruginosa, Staphylococcus aureus, and Streptococcus pneumonia, the treatment increased the relative abundance of P. aeruginosa while decreasing the Streptococcus spp. and P. melaninogenica. By Day 6, the community slowly recovered to the initial starting community structure. The results suggest that fluctuations of microbial profiles within a single patient are more likely due to community perturbations in the airways.
Given the consistency between the microbial profiles of 16S rDNA libraries and metagenomes from HL-derived DNA, we ruled out the biases originating from the 16S rRNA primers used in this study. One possible explanation for the differences seen across 16S rDNA taxonomical profiles generated from total DNA and HL-derived DNA (Figure 3B) may be the presence of high amounts of Pseudomonas spp. extracellular DNA after the antibiotic treatment. This is supported by the findings that these differences were most apparent at Day 7, three days after the antibiotics treatment, which targets Pseudomonas spp. in addition to others. Ciprofloxacin is commonly used as the first-line treatment in patients with CF and chronic P. aeruginosa infection even though its spectrum of activity includes most CF-associated pathogens. We hypothesized that the antibiotic treatment eradicates susceptible communities including Streptococcus spp. and hence creating a niche filled by resistant P. aeruginosa. Pseudomonas aeruginosa may gain resistance through increasing its biofilm communities and extracellular DNA has been shown to be the main structural support of its biofilm architecture52. Even as the community structure recovered, extracellular DNA may have remained in the CF sputum. Therefore, these data suggest that hypotonic lysis and the washing steps presented in this workflow potentially benefit in not only removing the human-derived DNA, but also microbial-derived extracellular DNA that may misrepresent the actual microbial profiles.
Metatranscriptomics
A high quality metatranscriptome should contain relatively few ribosomal RNA (rRNA) sequences and represent an unbiased sampling of the community transcripts (mRNA). Due to the short half-life and limited amount of mRNA, it is critical that the protocol, as presented here, minimizes sample handling to maximize the number of transcripts recovered.
In recent years, several approaches for rRNA depletion have been developed and adapted in commercially available kits. These include MICROBEnrich, Ribo-Zero, and sample-specific subtractive hybridizations53 that are based on oligonucleotide hybridization, and the mRNA-ONLY kit that is based on exonuclease enzymatic activity targeting RNA containing a 5&#8217; monophosphate. In addition, several approaches for mRNA enrichments such as the MessageAmp II-Bacteria Kit that preferentially polyadenylates and amplifies linear RNA are also available. Some of these methods (e.g., mRNA-ONLY, MICROBExpress and the MessageAmp) are used concurrently for optimal efficiency. However, the efficacy of all of these approaches are limited, especially when working with partially degraded rRNA, as often observed in total RNA extracted from CF samples. Polyadenylation-dependent RNA amplification cannot be used to generate metatranscriptomes consisting of both eukaryotic and prokaryotic mRNA. In addition, the poly(A) tail added to the sequences may reduces the amount of useful sequence data. Regions with homopolymer stretches will tend to have lower quality scores, causing a significant number of reads to be filtered out by sequencing and post-sequencing software, and the average useful read length after trimming off poly (A) tails will be reduced significantly54.
Dealing with complex CF microbial communities and partially degraded RNA (Figures 4A and 4C), our previous study showed that the hybridization-capture method by the Ribo-Zero Gold kit was more effective in removing both human and microbial rRNA compared to the combine treatments using other kits9 (Table 3). The resultant data allows concurrent analysis of both human host and microbial transcripts. Depending on the yield and quality of RNA, as well as ultimate choice of sequencing platform, many of these processes including the cDNA synthesis step can be streamlined with sequencing library generation. For example, Ribo-Zero treated RNA can be used to make metatranscriptome sequencing libraries using ScriptSeq RNA-Seq Library Preparation kit.
Metagenomic analysis of animal-associated communities provides a comprehensive representation of the overall functional entity that includes the host and its associated communities. The workflow presented here is adaptable to a variety of complex animal-associated samples, especially those that contain thick mucus, high amounts of cell debris, extracellular DNA, protein and glycoprotein complexes, as well as host cells in addition to the desired viral and microbial particles. Even though viral and microbial particles may be lost at every step, particles isolation and purification are essential to minimize the amount of host DNA. While the metagenomics data provides metabolic potentials of the communities examined, metatranscriptomics complement this by revealing the differential expression of encoded functions9. A comprehensive assessment of the genomics and transcripts data has yielded new insights to the dynamics of community interactions and facilitates the development of improving therapies9,10,55.

Viral and microbial communities associated with the human body have been investigated extensively in the past decade through the application of sequencing technologies1,2. The outcomes have led to the recognition of the importance microbes in human health and disease. The major initiative came from the human microbiome project that describes the bacteria (and some archaea) residing on human skin, and within oral cavities, airways, urogenital tract, and gastrointestinal tract3. Further microbiome studies of healthy human airways through bronchoalveolar lavage (BAL)4,5 and nasopharyngeal swabs4 have shown that the lung can serve as an environmental sampling device, results in transient microbial colonization in the airways. However, the impact of microbial colonization in impaired airway surfaces can lead to severe and chronic lung infections, such as those seen in Cystic Fibrosis (CF) patients.
CF is a lethal genetic disease caused by the mutation in Cystic Fibrosis Transmembrane Regulator (CFTR) gene6. These mutations give rise to defective CFTR proteins that in turn affect transepithelial ion transport across the apical surface of the epithelium. The disease affects multiple organ systems, but the majority of mortality and morbidity is attributable to CF lung disease7. The CF lung provides a unique ecosystem for microbial colonization. The defect in ion transport causes mucus to build up in the CF airways, creating microenvironments consisting of aerobic, microaerophilic, and anaerobic compartments anchored by a static nutrient-rich mucosal surface. This environment facilitates the colonization and proliferation of microbes, including viral, bacteria, and fungi. Acute and chronic pulmonary microbial infections lead to constant but ineffective immune responses, resulting in extensive airway remodeling, loss of pulmonary capacity, and ultimately pulmonary failure.
Bacterial communities associated with the CF lung have been well described using both culture-dependent and culture-independent approaches, which include using 16S ribosomal RNA (rRNA) gene sequencing8 and shotgun metagenomics9,10. The 16S rRNA-based approach is able to characterize a wide range of microbial species and capture broad shifts in community diversity. However, it is limited in its resolution in defining the communities (summarized in Claesson et al. 201011) and the predictions of metabolic potentials are limited to those general functions known for the taxa identified. Therefore, 16S rRNA gene sequencing methods are insufficient for the necessary taxonomic and functional analytic accuracy of the diverse microbial communities present in CF lungs. The metagenomic approach described here complements the 16S rRNA-based approach, overcomes its limitations, and enables a relatively effective way to analyze both the microbial community taxonomy and genetic contents in CF lungs.
Microbial DNA isolated from animal-associated samples often contains a large amount of host DNA. CF sputum or lung tissue samples usually contain a large amount of human DNA released by neutrophils in the immune response, often greater than 99% of the total DNA12&#8211;14. Although some intact human cells may be present, most of this DNA is free in solution or adsorbed to the surface of microbes. In addition, the presence of exceptionally viscous mucus plugs, cellular debris, and other unknown contaminants further complicate isolation of microbial cells. Several methods were tested for depleting these samples of human DNA, including Percoll gradients to separate human from microbial cells15, treatment with DNase I, ethidium bromide monoazide to selectively degrade human DNA16, and the MolYsis kit, all with limited success. To date the most effective microbial DNA purification procedure for CF sputum has been a modification of the process described by Breitenstein et al. (1995)17. This approach, herein known as hypotonic lysis (HL) method, uses a combination of &#946;-mercaptoethanol to reduce mucin disulfide bonds, hypotonic lysis of eukaryotic cells, and DNase I treatment of soluble DNA9. Despite the lack of alternatives the HL method raised some concerns due to (i) possible biases resulting from unwanted lysis of microbes and (ii) whether the observed fluctuations in community composition9,10 are an artifact of variations associated with the sample processing. In addition to the generation of shotgun metagenomes, we address these issues by comparing the 16S rRNA gene profiles of the total DNA and microbial DNA extracted from the HL method using the same set of sputum samples collected from a single patient across seven consecutive days.
Compared to microbial communities, the characterization of viral communities associated with animals is limited18,19. The viral communities in CF airways have only been characterized minimally20&#8211;22. The first metagenomic study characterizing the DNA of viral communities in CF airways showed that most viruses associated with CF lungs are phages20. The metabolic potential of phage in CF and non-CF individuals was significantly different. Specifically, the phage communities in CF individuals carried genes reflective of bacterial host adaptations to the physiology of CF airways, and bacterial virulence20. Subsequent metagenomic studies of viruses in CF lung tissue demonstrated distinct spatial heterogeneity of viral communities between anatomical regions22. In addition, CF lung tissue harbored the lowest viral diversity observed to date in any ecosystem22. Most viruses identified were phages with the potential to infect CF pathogens. However, eukaryotic viruses such as herpesviruses, adenoviruses, and human papilloma viruses (HPV) were also detected. In one event, where cysts in the lung tissue were observed during dissection, more than 99% of a human papillomavirus genome was recovered, even though the patient was never diagnosed with a pulmonary papilloma or carcinoma. This indicates that the viral diversity present not only reflects the severity of tissue damage, but may also expose and explain an underlying uncharacterized disease. The protocols described here provide a simple, yet powerful way to isolate viral-like particles (VLPs) from samples that consist of large amounts of thick mucus, host and microbial cells, free DNA, as well as cell debris.
Complementing metagenomics, metatranscriptomics is used to monitor the dynamics in gene expression across the microbial community and the host9,23. In this case, both microbial and host mRNA need to be preferentially selected. Since bacterial mRNAs are not polyadenylated, an oligo-dT-based mRNA pull-down method cannot be exploited. Polyadenylation-dependent RNA amplification cannot be used in host-associated samples if the samples are known to contain large amounts of eukaryotic mRNA. Many animal-associated samples, including CF sputum, contain a high density of cells in addition to high amounts of cellular debris and nucleases that include RNases. Therefore, another challenging task is to prevent extensive RNA degradation during metatranscriptome processing. In most cases, total RNA extracted from CF sputum is partially degraded, limiting the downstream applications and utility of the derived RNA. In recent years, several approaches for rRNA depletion have been developed and adapted in commercially available kits. The efficacy of these approaches is however limited, especially when working with partially degraded rRNA9,24. The methods employed here allowed for the retrieval of partially degraded total RNA suitable for efficient downstream total rRNA removal. Direct comparison of the efficiency in rRNA removal from partially degraded total RNA comparing two different kits was illustrated by Lim et al. (2012)9.
Overall, the goal of this manuscript is to provide a complete set of protocols (Figure 1) to generate viral and microbial shotgun metagenomes, and a metatranscriptome, from a single animal-associated sample, using induced sputum sample as an example. Molecular laboratory workflow should include separate pre- and post-amplification areas to minimize cross-contamination. The methods are easily adaptable to other sample types such as tissue22, nasopharyngeal and oropharyngeal swabs25, bronchoalveolar lavage (BAL) and coral (unpublished data). Each sample should be processed immediately upon collection especially when microbial metagenomics and metatranscriptomics studies are desired. If the samples were frozen, it limits the isolation of intact microbial cells for microbial metagenomes as freezing potentially disrupt the cell integrity. However, freezing does not preclude metatranscriptomics and viral isolation, but the quality of RNA and amount of viral particles recovered may be affected through the freeze-thaw process. It is important to note that induced sputum has served as the primary source of samples in many studies associated with adult CF patients and other chronic pulmonary diseases26,27 as BAL can be too invasive. In our studies, sputum samples were collected with a careful and consistent sampling method, i.e., following mouthwash and rinsing of the oral cavity using sterile saline solution to keep oral microbes contamination within the sputum samples to a minimum.

<table border="0" cellpadding="0" cellspacing="0" width="741">
	<tbody>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Name of Material/ Equipment</td>
			<td style="width:119px;">Company</td>
			<td style="width:119px;">Catalog Number</td>
			<td style="width:167px;">Comments/Description</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;">Guanidine isothiocyanate-based RNA lysis buffer</td>
			<td style="width:119px;">Life Technologies</td>
			<td>10296-028</td>
			<td>TRIzol LS Reagent was used in this study</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Silica beads; 0.1 to 0.15 mm</td>
			<td style="width:119px;">Cole-Parmer</td>
			<td>YO-36270-62</td>
			<td>Zirconia-Silicate Beads were used in this study</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Dithiothreitol Molecular Grade (Dry Powder)</td>
			<td style="width:119px;">Promega</td>
			<td style="width:119px;">V3155</td>
			<td>Can be purchased from any other company</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Sterile syringe filter; 0.45 &#181;m pore size hydrophilic PVDF membrane</td>
			<td style="width:119px;">Millipore</td>
			<td style="width:119px;">SLHV033RS</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">DNase I enzyme&#160;</td>
			<td>Calbiochem</td>
			<td align="right">260913</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Sterile syringe filter; 0.02 &#181;m pore size</td>
			<td style="width:119px;">FisherScientific</td>
			<td style="width:119px;">09-926-13</td>
			<td>Diameter: 25mm</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Ultra-Clear Centrifuge Tubes</td>
			<td style="width:119px;">Beckman</td>
			<td align="right">344059</td>
			<td>9/16 X 3 &#189; in. (14X90mm), suitable for SW41 Ti Rotor and VLPs density gradient ultracentrifugation</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">SW41 Ti Rotor</td>
			<td style="width:119px;">Beckman</td>
			<td align="right" style="width:119px;">333790</td>
			<td></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:337px;">SS-34 Fixed Angle Rotor</td>
			<td style="width:119px;">Thermo Scientific</td>
			<td align="right" style="width:119px;">28020</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Phi29 DNA polymerase</td>
			<td>Monserate Biotech</td>
			<td align="right" style="width:119px;">4001</td>
			<td>10 U/&#181;l</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Phi29 Random Hexamer</td>
			<td>Thermo Scientific</td>
			<td style="width:119px;">S0181</td>
			<td>Previously bought from Fidelity Systems</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Alumina matrix filter with annular polypropylene support ring; 0.02 &#181;m pore size</td>
			<td style="width:119px;">FisherScientific</td>
			<td style="width:119px;">09-926-34</td>
			<td>Whatman Anodisc Filter Membranes were used in this study; Diameter 25mm</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:337px;">SYBR Gold Nucleic Acid Gel Stain</td>
			<td style="width:119px;">Life Technologies</td>
			<td style="width:119px;">S-11494</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">2-Mercaptoethanol</td>
			<td style="width:119px;">Sigma-Aldrich</td>
			<td style="width:119px;">M6250-100ML</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">RNase-free DNase I&#160;</td>
			<td style="width:119px;">NEB</td>
			<td style="width:119px;">M0303S</td>
			<td>Can be purchased from any other company</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Glycogen, RNA grade</td>
			<td style="width:119px;">FisherScientific</td>
			<td style="width:119px;">FERR0551</td>
			<td>Can be purchased from any other company</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Oak Ridge high-speed centrifuge tubes</td>
			<td style="width:119px;">FisherScientific</td>
			<td style="width:119px;">05-562-16B</td>
			<td>For large volume DNA extraction procedure, suitable for SS-34 fixed-angle rotor</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Total rRNA removal kit</td>
			<td style="width:119px;">Epicentre</td>
			<td style="width:119px;">MRZE724</td>
			<td>ScriptSeq Complete Gold Kit (Epidemiology) can be used to couple rRNA removal with sequencing library preparation</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Cesium chloride&#160;</td>
			<td style="width:119px;">FisherScientific</td>
			<td style="width:119px;">BP1595-500</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:337px;">Hexadecytrimethyl-ammonium bromide (CTAB)</td>
			<td style="width:119px;">Sigma-Aldrich</td>
			<td style="width:119px;">H5882-100G</td>
			<td></td>
		</tr>
	</tbody>
</table>

purifying the impure: sequencing metagenomes and metatranscriptomes from complex animal-associated samples

The accessibility of high-throughput sequencing has revolutionized many fields of biology. In order to better understand host-associated viral and microbial communities, a comprehensive workflow for DNA and RNA extraction was developed. The workflow concurrently generates viral and microbial metagenomes, as well as metatranscriptomes, from a single sample for next-generation sequencing. The coupling of these approaches provides an overview of both the taxonomical characteristics and the community encoded functions. The presented methods use Cystic Fibrosis (CF) sputum, a problematic sample type, because it is exceptionally viscous and contains high amount of mucins, free neutrophil DNA, and other unknown contaminants. The protocols described here target these problems and successfully recover viral and microbial DNA with minimal human DNA contamination. To complement the metagenomics studies, a metatranscriptomics protocol was optimized to recover both microbial and host mRNA that contains relatively few ribosomal RNA (rRNA) sequences. An overview of the data characteristics is presented to serve as a reference for assessing the success of the methods. Additional CF sputum samples were also collected to (i) evaluate the consistency of the microbiome profiles across seven consecutive days within a single patient, and (ii) compare the consistency of metagenomic approach to a 16S ribosomal RNA gene-based sequencing. The results showed that daily fluctuation of microbial profiles without antibiotic perturbation was minimal and the taxonomy profiles of the common CF-associated bacteria were highly similar between the 16S rDNA libraries and metagenomes generated from the hypotonic lysis (HL)-derived DNA. However, the differences between 16S rDNA taxonomical profiles generated from total DNA and HL-derived DNA suggest that hypotonic lysis and the washing steps benefit in not only removing the human-derived DNA, but also microbial-derived extracellular DNA that may misrepresent the actual microbial profiles.

Watch this Scientific Journal Video about Purifying the Impure: Sequencing Metagenomes and Metatranscriptomes from Complex Animal-associated Samples at JoVE.com

Purifying the Impure: Sequencing Metagenomes and Metatranscriptomes from Complex Animal-associated Samples

Using the cystic fibrosis airway as an example, the manuscript presents a comprehensive workflow comprising a combination of metagenomic and metatranscriptomic approaches to characterize the microbial and viral communities in animal-associated samples.

The accessibility of high-throughput sequencing has revolutionized many fields of biology. In order to better understand host-associated viral and ...

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37.2K Views.  San Diego State University. Using the cystic fibrosis airway as an example, the manuscript presents a comprehensive workflow comprising a combination of metagenomic and metatranscriptomic approaches to characterize the microbial and viral communities in animal-associated samples.

Video: Purifying the Impure: Sequencing Metagenomes and Metatranscriptomes from Complex Animal-associated Samples

Purifying Plasmid DNA from Bacterial Colonies Using the Qiagen Miniprep Kit

Plasmid DNA purification from E. coli is a core technique for molecular cloning. Small scale purification (miniprep) from less than 5 ml of bacterial culture is a quick way for clone verification or DNA isolation, followed by further enzymatic reactions (polymerase chain reaction and restriction enzyme digestion). Here, we video-recorded the general procedures of miniprep through the QIAGEN's QIAprep 8 Miniprep Kit, aiming to introducing this highly efficient technique to the general beginners for molecular biology techniques. The whole procedure is based on alkaline lysis of E. coli cells followed by adsorption of DNA onto silica in the presence of high salt. It consists of three steps: 1) preparation and clearing of a bacterial lysate, 2) adsorption of DNA onto the QIAprep membrane, 3) washing and elution of plasmid DNA. All steps are performed without the use of phenol, chloroform, CsCl, ethidium bromide, and without alcohol precipitation. It usually takes less than 2 hours to finish the entire procedure.

Plasmid DNA purification from E. coli is a core technique for molecular cloning. Small scale purification (miniprep) from less than 5 ml of bacterial ...

Gross Dissection of the Stomach of the Lobster, Homarus Americanus

The stomach of the American lobster (Homarus americanus) is located in the cephalothorax, between the rostrum and the cervical groove. The anterior end of the stomach is defined by the mouth opening and the posterior end by the bottom of the pylorus. Along the dorsal side of the stomach lies the stomatogastric nervous system (STNS). This nervous system, which contains rhythmic networks that underlie feeding behavior, is an established model system for studying rhythm generating networks and neuromodulation 1,2. While it is possible to study this system in vivo 3, the STNS continues to produce its rhythmic activity when isolated in vitro. In order to study this system in vitro the stomach must be removed from the animal. This video article describes how the stomach can be dissected from the American lobster. In an accompanying video article4 we demonstrate how the STNS can be isolated from the stomach.

Gross Dissection of the Stomach of the Lobster, Homarus Americanus

We describe the gross dissection of the stomach of the American lobster (Homarus americanus).

The stomach of the American lobster (Homarus americanus) is located in the cephalothorax, between the rostrum and the cervical groove. The anterior end of ...

A Lectin HPLC Method to Enrich Selectively-glycosylated Peptides from Complex Biological Samples

Glycans are an important class of post-translational modifications. Typically found on secreted and extracellular molecules, glycan structures signal the internal status of the cell. Glycans on tumor cells tend to have abundant sialic acid and fucose moieties. We propose that these cancer-associated glycan variants be exploited for biomarker development aimed at diagnosing early-stage disease. Accordingly, we developed a mass spectrometry-based workflow that incorporates chromatography on affinity matrices formed from lectins, proteins that bind specific glycan structures. The lectins Sambucus nigra (SNA) and Aleuria aurantia (AAL), which bind sialic acid and fucose, respectively, were covalently coupled to POROS beads (Applied Biosystems) and packed into PEEK columns for high pressure liquid chromatography (HPLC). Briefly, plasma was depleted of the fourteen most abundant proteins using a multiple affinity removal system (MARS-14; Agilent). Depleted plasma was trypsin-digested and separated into flow-through and bound fractions by SNA or AAL HPLC. The fractions were treated with PNGaseF to remove N-linked glycans, and analyzed by LC-MS/MS on a QStar Elite. Data were analyzed using Mascot software. The experimental design included positive controls&mdash;fucosylated and sialylated human lactoferrin glycopeptides&mdash;and negative controls&mdash;high mannose glycopeptides from Saccharomyces cerevisiae&mdash;that were used to monitor the specificity of lectin capture. Key features of this workflow include the reproducibility derived from the HPLC format, the positive identification of the captured and PNGaseF-treated glycopeptides from their deamidated Asn-Xxx-Ser/Thr motifs, and quality assessment using glycoprotein standards. Protocol optimization also included determining the appropriate ratio of starting material to column capacity, identifying the most efficient capture and elution buffers, and monitoring the PNGaseF-treatment to ensure full deglycosylation. Future directions include using this workflow to perform mass spectrometry-based discovery experiments on plasma from breast cancer patients and control individuals.

Lectin-conjugated POROS beads were employed for HPLC. Glycopeptide standards served as positive and negative controls. MARS-14 depleted, trypsin-digested human plasma was chromatographed and flow-through (FT) and bound fractions collected for ESI-LC-MS/MS analyses. Glycopeptides were enriched in the bound fraction as compared to FT.

Glycans are an important class of post-translational modifications. Typically found on secreted and extracellular molecules, glycan structures signal the ...

Quantitation of &gamma;H2AX Foci in Tissue Samples

DNA double-strand breaks (DSBs) are particularly lethal and genotoxic lesions, that can arise either by endogenous (physiological or pathological) processes or by exogenous factors, particularly ionizing radiation and radiomimetic compounds. Phosphorylation of the H2A histone variant, H2AX, at the serine-139 residue, in the highly conserved C-terminal SQEY motif, forming &gamma;H2AX, is an early response to DNA double-strand breaks1. This phosphorylation event is mediated by the phosphatidyl-inosito 3-kinase (PI3K) family of proteins, ataxia telangiectasia mutated (ATM), DNA-protein kinase catalytic subunit and ATM and RAD3-related (ATR)2. Overall, DSB induction results in the formation of discrete nuclear &gamma;H2AX foci which can be easily detected and quantitated by immunofluorescence microscopy2. Given the unique specificity and sensitivity of this marker, analysis of &gamma;H2AX foci has led to a wide range of applications in biomedical research, particularly in radiation biology and nuclear medicine. The quantitation of &gamma;H2AX foci has been most widely investigated in cell culture systems in the context of ionizing radiation-induced DSBs. Apart from cellular radiosensitivity, immunofluorescence based assays have also been used to evaluate the efficacy of radiation-modifying compounds. In addition, &gamma;H2AX has been used as a molecular marker to examine the efficacy of various DSB-inducing compounds and is recently being heralded as important marker of ageing and disease, particularly cancer3. Further, immunofluorescence-based methods have been adapted to suit detection and quantitation of &gamma;H2AX foci ex vivo and in vivo4,5. Here, we demonstrate a typical immunofluorescence method for detection and quantitation of &gamma;H2AX foci in mouse tissues.

Quantitation of &#947;H2AX Foci in Tissue Samples

Quantitation of DNA double-strand breaks on the basis of &gamma;H2AX foci has become an invaluable tool, particularly in radiation biology, for the evaluation of tissue radiosensitivity and effects of radiation modifying compounds. Here we demonstrate the use of an immunofluorescence assay for quantitation of &gamma;H2AX foci in tissue samples.

DNA double-strand breaks (DSBs) are particularly lethal and genotoxic lesions, that can arise either by endogenous (physiological or pathological) ...

Chemically-blocked Antibody Microarray for Multiplexed High-throughput Profiling of Specific Protein Glycosylation in Complex Samples

In this study, we describe an effective protocol for use in a multiplexed high-throughput antibody microarray with glycan binding protein detection that allows for the glycosylation profiling of specific proteins. Glycosylation of proteins is the most prevalent post-translational modification found on proteins, and leads diversified modifications of the physical, chemical, and biological properties of proteins. Because the glycosylation machinery is particularly susceptible to disease progression and malignant transformation, aberrant glycosylation has been recognized as early detection biomarkers for cancer and other diseases. However, current methods to study protein glycosylation typically are too complicated or expensive for use in most normal laboratory or clinical settings and a more practical method to study protein glycosylation is needed. The new protocol described in this study makes use of a chemically blocked antibody microarray with glycan-binding protein (GBP) detection and significantly reduces the time, cost, and lab equipment requirements needed to study protein glycosylation. In this method, multiple immobilized glycoprotein-specific antibodies are printed directly onto the microarray slides and the N-glycans on the antibodies are blocked. The blocked, immobilized glycoprotein-specific antibodies are able to capture and isolate glycoproteins from a complex sample that is applied directly onto the microarray slides. Glycan detection then can be performed by the application of biotinylated lectins and other GBPs to the microarray slide, while binding levels can be determined using Dylight 549-Streptavidin. Through the use of an antibody panel and probing with multiple biotinylated lectins, this method allows for an effective glycosylation profile of the different proteins found in a given human or animal sample to be developed.
Introduction
Glycosylation of protein, which is the most ubiquitous post-translational modification on proteins, modifies the physical, chemical, and biological properties of a protein, and plays a fundamental role in various biological processes1-6. Because the glycosylation machinery is particularly susceptible to disease progression and malignant transformation, aberrant glycosylation has been recognized as early detection biomarkers for cancer and other diseases 7-12. In fact, most current cancer biomarkers, such as the L3 fraction of &alpha;-1 fetoprotein (AFP) for hepatocellular carcinoma 13-15, and CA199 for pancreatic cancer 16, 17 are all aberrant glycan moieties on glycoproteins. However, methods to study protein glycosylation have been complicated, and not suitable for routine laboratory and clinical settings. Chen et al. has recently invented a chemically blocked antibody microarray with a glycan-binding protein (GBP) detection method for high-throughput and multiplexed profile glycosylation of native glycoproteins in a complex sample 18. In this affinity based microarray method, multiple immobilized glycoprotein-specific antibodies capture and isolate glycoproteins from the complex mixture directly on the microarray slide, and the glycans on each individual captured protein are measured by GBPs. Because all normal antibodies contain N-glycans which could be recognized by most GBPs, the critical step of this method is to chemically block the glycans on the antibodies from binding to GBP. In the procedure, the cis-diol groups of the glycans on the antibodies were first oxidized to aldehyde groups by using NaIO4 in sodium acetate buffer avoiding light. The aldehyde groups were then conjugated to the hydrazide group of a cross-linker, 4-(4-N-MaleimidoPhenyl)butyric acid Hydrazide HCl (MPBH), followed by the conjugation of a dipeptide, Cys-Gly, to the maleimide group of the MPBH. Thus, the cis-diol groups on glycans of antibodies were converted into bulky none hydroxyl groups, which hindered the lectins and other GBPs bindings to the capture antibodies. This blocking procedure makes the GBPs and lectins bind only to the glycans of captured proteins. After this chemically blocking, serum samples were incubated with the antibody microarray, followed by the glycans detection by using different biotinylated lectins and GBPs, and visualized with Cy3-streptavidin. The parallel use of an antibody panel and multiple lectin probing provides discrete glycosylation profiles of multiple proteins in a given sample 18-20. This method has been used successfully in multiple different labs 1, 7, 13, 19-31. However, stability of MPBH and Cys-Gly, complicated and extended procedure in this method affect the reproducibility, effectiveness and efficiency of the method. In this new protocol, we replaced both MPBH and Cys-Gly with one much more stable reagent glutamic acid hydrazide (Glu-hydrazide), which significantly improved the reproducibility of the method, simplified and shorten the whole procedure so that the it can be completed within one working day. In this new protocol, we describe the detailed procedure of the protocol which can be readily adopted by normal labs for routine protein glycosylation study and techniques which are necessary to obtain reproducible and repeatable results.

In this study, we describe an improved protocol for a multiplexed high-throughput antibody microarray with lectin detection method that can be used in glycosylation profiling of specific proteins. This protocol features new reliable reagents and significantly reduces the time, cost, and lab equipment requirements as compared to the previous procedure.

 In this study, we describe an effective protocol for use in a multiplexed high-throughput antibody microarray with glycan binding protein detection that ...

Detection of Rare Genomic Variants from Pooled Sequencing Using SPLINTER

As DNA sequencing technology has markedly advanced in recent years2, it has become increasingly evident that the amount of genetic variation between any two individuals is greater than previously thought3. In contrast, array-based genotyping has failed to identify a significant contribution of common sequence variants to the phenotypic variability of common disease4,5. Taken together, these observations have led to the evolution of the Common Disease / Rare Variant hypothesis suggesting that the majority of the "missing heritability" in common and complex phenotypes is instead due to an individual's personal profile of rare or private DNA variants6-8. However, characterizing how rare variation impacts complex phenotypes requires the analysis of many affected individuals at many genomic loci, and is ideally compared to a similar survey in an unaffected cohort. Despite the sequencing power offered by today's platforms, a population-based survey of many genomic loci and the subsequent computational analysis required remains prohibitive for many investigators.
To address this need, we have developed a pooled sequencing approach1,9 and a novel software package1 for highly accurate rare variant detection from the resulting data. The ability to pool genomes from entire populations of affected individuals and survey the degree of genetic variation at multiple targeted regions in a single sequencing library provides excellent cost and time savings to traditional single-sample sequencing methodology. With a mean sequencing coverage per allele of 25-fold, our custom algorithm, SPLINTER, uses an internal variant calling control strategy to call insertions, deletions and substitutions up to four base pairs in length with high sensitivity and specificity from pools of up to 1 mutant allele in 500 individuals. Here we describe the method for preparing the pooled sequencing library followed by step-by-step instructions on how to use the SPLINTER package for pooled sequencing analysis (<a href="http://www.ibridgenetwork.org/wustl/splinter" target="_blank">http://www.ibridgenetwork.org/wustl/splinter</a>). We show a comparison between pooled sequencing of 947 individuals, all of whom also underwent genome-wide array, at over 20kb of sequencing per person. Concordance between genotyping of tagged and novel variants called in the pooled sample were excellent. This method can be easily scaled up to any number of genomic loci and any number of individuals. By incorporating the internal positive and negative amplicon controls at ratios that mimic the population under study, the algorithm can be calibrated for optimal performance. This strategy can also be modified for use with hybridization capture or individual-specific barcodes and can be applied to the sequencing of naturally heterogeneous samples, such as tumor DNA.

Pooled DNA sequencing is a fast and cost-effective strategy to detect rare variants associated with complex phenotypes in large cohorts. Here we describe the computational analysis of pooled, next-generation sequencing of 32 cancer-related genes using the SPLINTER software package. This method is scalable, and applicable to any phenotype of interest.

As DNA sequencing technology has markedly advanced in recent years2, it has become increasingly evident that the amount of genetic variation between any ...

The MultiBac Protein Complex Production Platform at the EMBL

Proteomics research revealed the impressive complexity of eukaryotic proteomes in unprecedented detail. It is now a commonly accepted notion that proteins in cells mostly exist not as isolated entities but exert their biological activity in association with many other proteins, in humans ten or more, forming assembly lines in the cell for most if not all vital functions.1,2 Knowledge of the function and architecture of these multiprotein assemblies requires their provision in superior quality and sufficient quantity for detailed analysis. The paucity of many protein complexes in cells, in particular in eukaryotes, prohibits their extraction from native sources, and necessitates recombinant production. The baculovirus expression vector system (BEVS) has proven to be particularly useful for producing eukaryotic proteins, the activity of which often relies on post-translational processing that other commonly used expression systems often cannot support.3 BEVS use a recombinant baculovirus into which the gene of interest was inserted to infect insect cell cultures which in turn produce the protein of choice. MultiBac is a BEVS that has been particularly tailored for the production of eukaryotic protein complexes that contain many subunits.4 A vital prerequisite for efficient production of proteins and their complexes are robust protocols for all steps involved in an expression experiment that ideally can be implemented as standard operating procedures (SOPs) and followed also by non-specialist users with comparative ease. The MultiBac platform at the European Molecular Biology Laboratory (EMBL) uses SOPs for all steps involved in a multiprotein complex expression experiment, starting from insertion of the genes into an engineered baculoviral genome optimized for heterologous protein production properties to small-scale analysis of the protein specimens produced.5-8 The platform is installed in an open-access mode at EMBL Grenoble and has supported many scientists from academia and industry to accelerate protein complex research projects.

Protein complexes catalyze key cellular functions. Detailed functional and structural characterization of many essential complexes requires recombinant production. MultiBac is a baculovirus/insect cell system particularly tailored for expressing eukaryotic proteins and their complexes. MultiBac was implemented as an open-access platform, and standard operating procedures developed to maximize its utility.

Proteomics  research revealed the impressive complexity of eukaryotic proteomes in  unprecedented detail. It is now a commonly accepted notion that ...

High Yield Expression of Recombinant Human Proteins with the Transient Transfection of HEK293 Cells in Suspension

The art of producing recombinant proteins with complex post-translational modifications represents a major challenge for studies of structure and function. The rapid establishment and high recovery from transiently-transfected mammalian cell lines addresses this barrier and is an effective means of expressing proteins that are naturally channeled through the ER and Golgi-mediated secretory pathway. Here is one protocol for protein expression using the human HEK293F and HEK293S cell lines transfected with a mammalian expression vector designed for high protein yields. The applicability of this system is demonstrated using three representative glycoproteins that expressed with yields between 95-120 mg of purified protein recovered per liter of culture. These proteins are the human Fc&#947;RIIIa and the rat &#945;2-6 sialyltransferase, ST6GalI, both expressed with an N-terminal GFP fusion, as well as the unmodified human immunoglobulin G1 Fc. This robust system utilizes a serum-free medium that is adaptable for expression of isotopically enriched proteins and carbohydrates for structural studies using mass spectrometry and nuclear magnetic resonance spectroscopy. Furthermore, the composition of the N-glycan can be tuned by adding a small molecule to prevent certain glycan modifications in a manner that does not reduce yield.

Laboratory-scale production of eukaryotic proteins with appropriate post-translational modification represents a significant barrier. Here is a robust protocol with rapid establishment and turnaround for protein expression using a mammalian expression system. This system supports selective amino acid, selective labeling of proteins and small molecule modulators of glycan composition.

The art of producing recombinant proteins with complex post-translational modifications represents a major challenge for studies of structure and ...

Amplification, Next-generation Sequencing, and Genomic DNA Mapping of Retroviral Integration Sites

Retroviruses exhibit signature integration preferences on both the local and global scales. Here, we present a detailed protocol for (1) generation of diverse libraries of retroviral integration sites using ligation-mediated PCR (LM-PCR) amplification and next-generation sequencing (NGS), (2) mapping the genomic location of each virus-host junction using BEDTools, and (3) analyzing the data for statistical relevance. Genomic DNA extracted from infected cells is fragmented by digestion with restriction enzymes or by sonication. After suitable DNA end-repair, double-stranded linkers are ligated onto the DNA ends, and semi-nested PCR is conducted using primers complementary to both the long terminal repeat (LTR) end of the virus and the ligated linker DNA. The PCR primers carry sequences required for DNA clustering during NGS, negating the requirement for separate adapter ligation. Quality control (QC) is conducted to assess DNA fragment size distribution and adapter DNA incorporation prior to NGS. Sequence output files are filtered for LTR-containing reads, and the sequences defining the LTR and the linker are cropped away. Trimmed host cell sequences are mapped to a reference genome using BLAT and are filtered for minimally 97% identity to a unique point in the reference genome. Unique integration sites are scrutinized for adjacent nucleotide (nt) sequence and distribution relative to various genomic features. Using this protocol, integration site libraries of high complexity can be constructed from genomic DNA in three days. The entire protocol that encompasses exogenous viral infection of susceptible tissue culture cells to integration site analysis can therefore be conducted in approximately one to two weeks. Recent applications of this technology pertain to longitudinal analysis of integration sites from HIV-infected patients.

We describe a protocol for amplifying retroviral integration sites from the genomic DNA of infected cells, sequencing the amplified virus-host junctions, and then mapping these sequences to a reference genome. We also describe techniques to quantify the distribution of integration sites relative to various genomic annotations using BEDTools.

Retroviruses exhibit signature integration preferences on both the local and global scales. Here, we present a detailed protocol for (1) generation of ...

Targeted RNA Sequencing Assay to Characterize Gene Expression and Genomic Alterations

RNA sequencing (RNAseq) is a versatile method that can be utilized to detect and characterize gene expression, mutations, gene fusions, and noncoding RNAs. Standard RNAseq requires 30 - 100 million sequencing reads and can include multiple RNA products such as mRNA and noncoding RNAs. We demonstrate how targeted RNAseq (capture) permits a focused study on selected RNA products using a desktop sequencer. RNAseq capture can characterize unannotated, low, or transiently expressed transcripts that may otherwise be missed using traditional RNAseq methods. Here we describe the extraction of RNA from cell lines, ribosomal RNA depletion, cDNA synthesis, preparation of barcoded libraries, hybridization and capture of targeted transcripts and multiplex sequencing on a desktop sequencer. We also outline the computational analysis pipeline, which includes quality control assessment, alignment, fusion detection, gene expression quantification and identification of single nucleotide variants. This assay allows for targeted transcript sequencing to characterize gene expression, gene fusions, and mutations.

We describe a targeted RNA sequencing-based method that includes preparation of indexed cDNA libraries, hybridization and capture with custom probes and data analysis to interrogate selected transcripts for gene expression, mutations, and gene fusions. Targeted RNAseq permits cost-effective, rapid evaluation of selected transcripts on a desktop sequencer.

RNA sequencing (RNAseq) is a versatile method that can be utilized to detect and characterize gene expression, mutations, gene fusions, and noncoding ...