This study was supported by Swedish Research Council (www.vr.se) grants to ARC (2014-6466 and the Swedish Foundation for Strategic Research (www.stratresearch.se) to ARC (ICA14-0060). Chalmers University of Technology provided financial support to MKME during this work. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.

This protocol is outlined in Figure 1 and includes the isolation of gDNA, digestion with restriction enzymes to be able to quantitate the number of ribonucleotides, treatment with alkali to hydrolyze the phosphodiester bonds of ribonucleotides incorporated into the gDNA, phosphorylation of free 5&#180;-OH ends, ssDNA ligation of adapters, second strand synthesis, and PCR amplification before sequencing.
1. Adapters and Index Primers
<ol>
	<li>Obtain ARC49, ARC140 oligonucleotides, ARC76/77, adapter and ARC78-ARC107 index primers (see Table 1). 
	NOTE: Oligonucleotides should be HPLC purified. ARC76/77 are ordered as duplex.</li>
	<li>Prepare 100 &#181;M stock solutions of each oligonucleotide in Tris-EDTA (TE) buffer (see the Table of Materials) and store at -20 &#176;C.</li>
	<li>Prepare 10 &#181;M solutions of ARC67/77 and 2 &#181;M solutions of ARC49 and index primers by diluting in elution buffer (EB; see the Table of Materials). Store at -20 &#176;C.</li>
</ol>
2. Growth and Harvest of Cells
<ol>
	<li>Grow HeLa cells in 70 mL Dulbecco&#39;s Modified Eagle Medium (DMEM) supplemented with 10% fetal bovine serum in a 250 mL Spinner flask at 37 &#176;C.</li>
	<li>Count the number of cells and collect 5x106 cells in a 50-mL tube, centrifuge for 5 min at 200 x g, and discard the supernatant.</li>
	<li>Wash the cells with 20 mL 1x PBS, centrifuge for 5 min at 200 x g, and discard the supernatant.</li>
	<li>Freeze the pellets at -20 &#176;C or continue with DNA purification.</li>
</ol>
3. DNA Purification and Quantitation
<ol>
	<li>Purify gDNA using phenol-chloroform extraction as described below.
	<ol>
		<li>Resuspend the cells in 2 mL lysis buffer (see the Table of Materials) and incubate for 30 min at 42 &#176;C on a heating block. 
		CAUTION: Lysis buffer contains hazardous components. SDS solution is irritating, Proteinase K is sensitizing, irritating, and toxic. Wear protective clothes and gloves.</li>
		<li>Split the sample in two 2 mL tubes and add 1 volume (V) of phenol-chloroform-isoamyl alcohol (25:24:1). 
		CAUTION: Phenol-chloroform-isoamyl alcohol is toxic, mutagenic, corrosive, and hazardous to aquatic environments. Use in a fume hood, wear protective clothes and gloves, and discard in special phenol-chloroform waste.</li>
		<li>Mix by inversion for 30-60 s and centrifuge for 5 min at 15,000 x g at room temperature. 
		NOTE: Do not vortex DNA to avoid introducing random strand breaks, which would distort the results.</li>
		<li>Transfer the upper, aqueous phase to a new 2 mL tube and add 1 V of phenol-chloroform-isoamyl alcohol (25:24:1).</li>
		<li>Mix by inversion and centrifuge for 5 min at 15,000 x g at 4 &#176;C.</li>
		<li>Transfer upper, aqueous phase to a new 2 mL tube and add 20 &#181;L NaCl (5 M) and 1 V of cold isopropanol. 
		CAUTION: Isopropanol is flammable, irritating, and toxic. Store it in a ventilated cabinet, wear protective clothes and gloves, and keep it away from flames.</li>
		<li>Mix by inversion and incubate for at least 1 h at -20 &#176;C.</li>
		<li>Centrifuge for 20 min at 15,000 x g, 4 &#176;C and discard supernatant.</li>
		<li>Wash DNA pellet with 200 &#181;L cold 70% ethanol, centrifuge for 20 min at 15,000 x g at 4 &#176;C and discard supernatant. 
		CAUTION: 70% ethanol is flammable and irritating. Keep working solution at -20 &#176;C, otherwise store in ventilated cabinet, wear protective clothes and gloves, and keep it away from flames.</li>
		<li>Dry the DNA pellet at room temperature for 20-25 min.</li>
		<li>Dissolve DNA pellets in 100 &#181;L TE buffer and pool the samples in one tube.</li>
	</ol>
	</li>
	<li>Quantitate DNA concentration using a dsDNA quantitation reagent according to manufacturer&#39;s specifications (see the Table of Materials). 
	NOTE: Use a dsDNA quantitation reagent, because spectrophotometric DNA quantitation can be affected by residual phenol.</li>
	<li>Store DNA at -20 &#176;C or continue with HincII treatment.</li>
</ol>
4. HincII Treatment and Alkaline Hydrolysis
<ol>
	<li>Digest 1 &#181;g of DNA in a reaction mix containing 5 &#181;L 10x buffer 3.1, 1 &#181;L (10 U) HincII, and nuclease-free H2O to a final volume of 50 &#181;L. 
	NOTE: To achieve optimal conditions for ligation, second strand synthesis and PCR amplification, it may be necessary to increase the amount of input DNA if it is expected that the DNA contains a very low number of ribonucleotides. Similarly, it may be necessary to decrease input DNA if the number of ribonucleotides is very high.</li>
	<li>Incubate for 30 min at 37 &#176;C.</li>
	<li>Purify HincII treated DNA with paramagnetic beads. 
	NOTE: Keep the tube lids open in the following steps to not disturb pellets by opening the tubes.
	<ol>
		<li>Add 1.8 V of paramagnetic beads to each sample, carefully mix by pipetting, and incubate at room temperature for 10 min.</li>
		<li>Use a magnetic rack to pellet the beads for 5 min, then remove and discard supernatant.</li>
		<li>Wash the pellet with 150 &#181;L of 70% ethanol (room temperature) for about 30 s then remove and discard the supernatant.</li>
		<li>Wash the pellet with 200 &#181;L of 70% ethanol (room temperature) for about 30 s then remove and discard the supernatant. 
		NOTE: Residual ethanol can be removed with a 10 &#181;L pipette. Droplets can be spun down briefly beforehand.</li>
		<li>Dry the samples at room temperature for around 15-20 min. 
		NOTE: The exact time depends on the volume of beads and the shape of the pellet, therefore the pellets should be checked visually.</li>
		<li>Remove tubes from the magnetic rack and elute pellet in 45 &#181;L EB, mix by pipetting carefully.</li>
		<li>Incubate for 5 min then pellet the beads on the magnetic rack and use 45 &#181;L of purified DNA in step 4.4.</li>
	</ol>
	</li>
	<li>Add 5 &#181;L of KOH (3 M) or KCl (3 M) to the DNA creating a total volume of 50 &#181;L. 
	CAUTION: 3 M KOH solution is corrosive. Wear protective clothes and gloves.</li>
	<li>Incubate for 2 h at 55 &#176;C in a hybridization oven followed by 5 min on ice. 
	NOTE: It is recommended to perform the KOH treatment in an oven rather than a heating block to maintain a uniform heating of the tube and prevent condensation at the lid.</li>
	<li>Precipitate DNA by adding 10 &#181;L sodium acetate (3 M, pH = 5.2) and 125 &#181;L cold 100% ethanol. Incubate on ice for 5 min. 
	CAUTION: 100% ethanol is flammable and irritating. Store in a ventilated cabinet, wear protective clothes and gloves, and keep away from flames.</li>
	<li>Pellet gDNA by centrifuging at 21,000 x g, 4 &#176;C for 5 min and discard the supernatant.</li>
	<li>Wash DNA pellet with 250 &#181;L cold 70% EtOH, centrifuge at 21,000 x g, 4 &#176;C for 5 min, and discard the supernatant. 
	NOTE: To remove droplets, the tube can be spun down briefly again and supernatant can be removed with a 10 &#181;l pipette.</li>
	<li>Let the pellet dry in an open tube for about 5-10 min until any visible fluid has evaporated.</li>
	<li>Let DNA pellet dissolve in 20 &#181;L EB for 30 min at room temperature.</li>
</ol>
5. 5&#180; End Phosphorylation
<ol>
	<li>Prepare the reaction mix for each sample in advance consisting of 2.5 &#181;L 10x T4 polynucleotide kinase reaction buffer, 1 &#181;L (10 U) 3&#180;-phosphatase-minus T4 polynucleotide kinase, and 2.5 &#181;L ATP (10 mM).</li>
	<li>Transfer 19 &#181;L of each DNA sample into a new 200 &#181;L tube and denature for 3 min at 85 &#176;C in a thermo-cycler.</li>
	<li>Cool DNA samples on ice and add 6 &#181;L of reaction mix to each sample.</li>
	<li>Incubate reaction mixes at 37 &#176;C for 30 min and stop the reaction by incubating the samples at 65 &#176;C for 20 min.</li>
	<li>Purify DNA as described in 4.3, using 1.8 V of paramagnetic beads but elute in 14 &#181;L EB.</li>
</ol>
6. ssDNA Ligation
<ol>
	<li>Prepare the reaction mix for each sample in advance consisting of 0.5 &#181;L ATP (2 mM), 5 &#181;L 10x T4 RNA ligase reaction buffer, 5 &#181;L CoCl3(NH3)6 (10 mM), 0.5 &#181;L ARC140 (100 &#181;M), and 25 &#181;L 50% PEG 8000. Mix well by pipetting. 
	CAUTION: CoCl3(NH3)6 is carcinogenic, sensitizing, and hazardous to aquatic environment. Wear protective clothes and gloves.</li>
	<li>Transfer 13 &#181;L of purified DNA from step 5.5 to a new 200 &#181;L tube and denature for 3 min at 85 &#176;C in a thermo-cycler.</li>
	<li>Cool the DNA on ice and add 36 &#181;L of reaction mix to each sample, mix by pipetting, and spin down briefly.</li>
	<li>Add 1 &#181;L (10 U) of T4 RNA Ligase to each reaction, mix by pipetting, and spin down briefly.</li>
	<li>Incubate the samples at room temperature in the dark overnight.</li>
</ol>
7. Second-strand Synthesis
<ol>
	<li>Purify ligated DNA as described in 4.3, but use 0.8 V of paramagnetic beads, pellet the beads for 10 min and elute in 20 &#181;L EB. 
	NOTE: Due to the higher viscosity of the ligation reaction mix, the first pelleting step is prolonged.</li>
	<li>Transfer 20 &#181;L of DNA sample to a new 200 &#181;L PCR tube. Repeat the purification step using 0.8 V of paramagnetic beads following the manufacturer&#39;s specifications and elute in 14 &#181;L EB.</li>
	<li>Prepare the reaction mix for each sample in advance consisting of 2 &#181;L of 10x T7 DNA polymerase reaction buffer, 2 &#181;L ARC76/77 (2 &#181;M), 2 &#181;L dNTPs (2 mM), and 0.8 &#181;L BSA (1 mg/mL).</li>
	<li>Transfer 12.8 &#181;L purified DNA to a new 200 &#181;L tube, denature for 3 min at 85 &#176;C in a thermo-cycler.</li>
	<li>Cool the DNA on ice and add 6.8 &#181;L of reaction mix to each sample, mix by pipetting, spin down briefly, and incubate for 5 min at room temperature.</li>
	<li>Add 0.4 &#181;L (4 U) T7 DNA polymerase to each reaction and incubate for 5 min at room temperature.</li>
	<li>Purify DNA as described in 4.3, using 0.8 V of paramagnetic beads and elute in 11 &#181;L EB.</li>
</ol>
8. PCR Amplification and Library Quantitation
<ol>
	<li>Prepare the reaction mix for each sample in a new 200 &#181;L tube in advance consisting of 7.5 &#181;L ARC49 (2 &#181;M), 7.5 &#181;L index primer (2 &#181;M, unique for each sample), and 25 &#181;L 2x hot start ready mix.</li>
	<li>Add 10 &#181;L of DNA sample to each reaction. Amplify the library using the following conditions: denature at 95 &#176;C for 45 s, followed by 18 cycles of 98 &#176;C for 15 s, 65 &#176;C for 30 s, 72 &#176;C for 30 s, ending with a final elongation at 72 &#176;C for 2 min. Hold samples at 4 &#176;C after amplification.</li>
	<li>Purify libraries as described in 4.3, using 0.8 V of paramagnetic beads, and elute in 20 &#181;L TE buffer.</li>
	<li>Quantitate libraries using a dsDNA quantitation reagent, according to the manufacturer&#39;s specifications (see the Table of Materials).</li>
	<li>Store samples at -20 &#176;C or continue with library analysis.</li>
</ol>
9. Library Analysis and Pooling
<ol>
	<li>Determine the quality of each library and estimate the average fragment size using a digital electrophoresis system. 
	NOTE: The average fragment size is assessed by estimating where the area under the curve of the electropherogram is halved, disregarding peaks from markers. Representative results of suitable library profiles after KOH or KCl treatment are given in Figure 2A.</li>
	<li>Calculate the concentration (nM) of the libraries as: 
	(c/103)/(p*650)]*109 
	where c is the concentration of the library in ng/&#181;L and p is the average fragment size in bp, as estimated in 9.1.</li>
	<li>Pool equal molar amounts of up to 24 libraries amplified with different index primers for sequencing. Add TE buffer to a final volume of 25 &#181;L and concentration of 10 nM. 
	NOTE: Depending on the number of libraries to be pooled, the amount of DNA from each library is adjusted. If primer dimers were detected in step 9.1 as a distinct peak of about 130 bp, the final volume of the library pool can exceed 25 &#181;L, because the purification step is repeated as described in 4.3, using 0.8 V of paramagnetic beads, and DNA is eluted in 25 &#181;L TE buffer.
	<ol>
		<li>Determine the new library pool concentration using a dsDNA quantitation reagent according to manufacturer&#39;s specifications and the average peak size as described above. Proceed to sequencing and data analysis (sections 10 and 11).</li>
	</ol>
	</li>
</ol>
10. Sequencing
<ol>
	<li>Perform 75-base paired-end sequencing on pooled libraries12.</li>
</ol>
11. Data Analysis
<ol>
	<li>Trim all reads to remove adapter sequences, filter for quality and read length. 
	NOTE: This can be done using cutadapt 1.2.120 with the command `cutadapt -f fastq --match-read-wildcards --quiet -m 15 -q 10 -a NNNNNNN &#60;FILE&#62;`, where NNNNNNN is replaced with the actual adapter sequence and &#60;FILE&#62; is replaced with the fastq file name.</li>
	<li>Remove mates of reads that were discarded in the previous step using custom scripts.</li>
	<li>Align Mate 1 of remaining pairs to an index containing the sequence of all oligonucleotides used in the library preparation (e.g., using Bowtie 0.12.821 and the command line options -m1 -v2). Discard all pairs with successful alignments.</li>
	<li>Align remaining pairs to the organism reference genome using Bowtie with the command line options -v2 -X10000--best.</li>
	<li>Map reads that span between the mitochondrial molecule beginning and end by aligning Mate 1 of all unaligned pairs (using Bowtie with the command line options -v2).</li>
	<li>Determine the count of 5&#180;-ends for all single and paired end alignments. Shift the position of these by one base upstream to the position where the hydrolyzed ribonucleotides were.</li>
	<li>Export data from the bowtie file format to a bedgraph file format using custom scripts for visualization in common genome browsers. Normalize the reads for each strand to reads per million.</li>
	<li>Using the position and counts from the bedgraph file, reference the organism genome sequence to determine the identity of incorporated ribonucleotides. 
	NOTE: For the human mitochondrial genome reads from the regions 16,200-300 and 5,747-5,847 for each strand should be excluded since these regions contain many free 5&#180;-ends unrelated to ribonucleotide incorporation by DNA polymerase &#947;.</li>
	<li>Divide the total reads, not including reads at the eleven HincII sites, with the mean number of reads per HincII site to get the number of ribonucleotides per single strand break, (i.e. the number of ribonucleotides per mitochondrial molecule).</li>
</ol>

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The authors declare that they have no competing financial interests.

Here we present a technique to simultaneously map and quantify ribonucleotides in gDNA, and mtDNA in particular, by the simple introduction of DNA cleavage at sequence specific sites in the genome as an addition to the established HydEn-seq protocol. While this study focuses on human mtDNA, originally the HydEn-seq method was developed in Saccharomyces cerevisiae, illustrating the method&#39;s translation to other organisms12,16.
For reliable results obtained from this approach, some critical steps should be noted: (A) Since sequencing adapters ligate to all available 5&#180;-ends, it is crucial to work with highly intact DNA. DNA should be isolated and libraries should be made preferably immediately after DNA isolation, or the DNA can be stored at -20 &#176;C. It is not recommended to store DNA in the fridge for a long time or to repeatedly freeze and thaw it. (B) To generate suitable libraries with this method, it is crucial to perform the KOH treatment of the DNA in an incubation oven, rather than a heating block, assuring homogenous heating of the whole sample and quantitative hydrolysis. (C) Furthermore, it is critical to control the quality of libraries before pooling and sequencing. The DNA should be quantified and analyzed using an automated electrophoresis system to ensure adequate amounts of library DNA, confirm appropriate fragment sizes, and check for primer dimers.
For a meaningful data analysis, it is also important to note that the informative value of this method is dependent on appropriate controls to assess background counts and sequence or strand biases. We routinely achieve a mapping efficiency in KCl samples of close to 70% when only digesting with the sequence specific endonuclease (Figure 2B, left panels). In addition, it is important to confirm that the endonuclease treatment is not affecting the overall detection of incorporated ribonucleotides by comparing HincII treated and untreated samples (Figure 3B). In these experiments, we have used HincII to introduce site specific cuts, though other high-fidelity restriction enzymes could also be used.
The protocol could be adapted to study other types of DNA lesions that can be processed to 5&#180;-phosphate or 5&#180;-OH ends. The accuracy of the results is dependent on the specificity of processing and requires suitable controls (e.g., wild type or untreated) for verification. Moreover, when adapting this method to other applications or for use with other organisms, one should consider that the method in its current setup requires about 1 &#181;g of DNA which is processed to a library. Since the number of ends is dependent on the number of embedded ribonucleotides, which varies depending on the organism or mutant, samples including a lower number of ribonucleotides would require more input DNA to generate a sufficient number of ends in the subsequent library construction. Similarly, if DNA samples have a much higher number of ribonucleotides, it would also require using less input DNA to obtain optimal conditions for ligation, second strand synthesis, and PCR amplification. It is noteworthy that the library construction as described in this protocol also generated data covering the nuclear genome (as displayed in Figure 2D) and only the data analysis was focused on mtDNA. This illustrates that larger genomes with moderately lower ribonucleotide frequencies are also captured by this method.
When considering this method, certain limitations should be taken into account: Although this method should, in theory, be applicable to virtually any organism, a suitable reference genome is necessary for the alignment of reads. Furthermore, the results obtained from our protocol represent the reads from a large number of cells. Specific ribonucleotide incorporation patterns of a subset of cells cannot be identified by this approach. If ribonucleotides are mapped in larger genomes with a very low number of ribonucleotides, it may be challenging to discriminate ribonucleotides from random nicks and appropriate controls are therefore needed.
The method we describe here, extends the available in vivo techniques such as HydEn-Seq16, Ribose-Seq17, Pu-Seq18, or emRiboSeq19. These approaches take advantage of the embedded ribonucleotides&#39; sensitivity to alkaline or RNase H2 treatment, respectively, employing Next-generation sequencing to identify ribonucleotides genome-wide, which allows their mapping and the comparison of relative incorporation. By cleaving the DNA sequence specifically, as described above, in addition to alkaline hydrolysis at embedded ribonucleotides, the reads for ribonucleotides can be normalized to those cleavage sites, allowing not only the identification and mapping of ribonucleotides, but also their quantitation for each DNA molecule. The application of our technique in the context of diseases related to DNA replication, DNA repair, and TLS could provide a deeper understanding of the role of ribonucleotides in underlying molecular mechanisms and genome integrity in general.

In a eukaryotic cell, the concentration of ribonucleotides (rNTPs) is much higher than the concentration of deoxyribonucleotides (dNTPs)1. DNA polymerases discriminate against ribonucleotides, but this discrimination is not perfect and, as a consequence, ribonucleotides instead of deoxyribonucleotides may be incorporated into genomes during DNA replication. Ribonucleotides may be the most common non-canonical nucleotides incorporated into the genome2. Most of these ribonucleotides are removed during Okazaki fragment maturation by RNase H2 initiated ribonucleotide excision repair (RER) or by Topoisomerase 1 (reviewed in reference3). Ribonucleotides that cannot be removed stay stably incorporated in the DNA2,4 and may affect it in both harmful and beneficial ways (reviewed in reviewed5). Besides being able to act as positive signals, for example in mating type switch in Schizosaccharomyces pombe6 and marking the nascent DNA strand during mismatch repair (MMR)7,8, ribonucleotides affect the structure9 and stability of the surrounding DNA due to the 2&#180;-hydroxyl group of their ribose10, resulting in replicative stress and genome instability11. The abundance of ribonucleotides in genomic DNA (gDNA) and their relevance in replication and repair mechanisms, as well as the implications for genome stability, give reason to investigate their precise occurrence and frequency in a genome-wide manner.
RNase H2 activity has not been found in human mitochondria and ribonucleotides are therefore not efficiently removed in mitochondrial DNA (mtDNA). Several pathways are involved in the supply of nucleotides to human mitochondria and to investigate whether disturbances in the mitochondrial nucleotide pool cause an elevated number of ribonucleotides in human mtDNA, we developed a protocol to map and quantitate these ribonucleotides in human mtDNA isolated from fibroblasts, HeLa cells, and patient cell lines12.
Most in vitro approaches (reviewed in reviewed13) to determine DNA polymerases&#39; selectivity against rNTPs are based on single ribonucleotide insertion or primer extension experiments where competing rNTPs are included in the reaction mix, allowing the identification or relative quantitation of ribonucleotide incorporation in short DNA templates. Quantitative approaches on short sequences may not reflect dNTP and rNTP pools at cellular concentrations and therefore provide insight into polymerase selectivity but are of limited significance regarding whole genomes. It has been shown that the relative amount of ribonucleotides incorporated during the replication of a longer DNA template, such as a plasmid, can be visualized on a sequencing gel using radiolabeled dNTPs and hydrolyzing the DNA in an alkaline milieu14. Furthermore, gDNA has been analyzed on Southern blots following alkaline hydrolysis, allowing strand-specific probing and determination of absolute rates of ribonucleotide incorporation in vivo15. These approaches allow a relative comparison of incorporation frequency but deliver no insight into the position or identity of the incorporated ribonucleotides. More recent approaches to analyze the ribonucleotide content in gDNA in vivo, like HydEn-Seq16, Ribose-Seq17, Pu-Seq18, or emRiboSeq19, take advantage of the embedded ribonucleotides&#39; sensitivity to alkaline or RNase H2 treatment, respectively, and employ Next-generation sequencing to identify ribonucleotides genome-wide. These methods do not provide insight into the absolute incorporation frequency of the detected ribonucleotides. By adding the step of sequence specific enzymatic cleavage to the HydEn-seq protocol, the method we describe here conveniently extends the information gained from a sequencing approach, allowing simultaneous mapping and quantitation of embedded ribonucleotides12. This method is applicable to virtually any organism given that highly intact DNA extracts can be generated and a suitable reference genome is available. The method could be adapted to quantitate and determine the location of any lesion that can be digested by a nuclease and leaves a 5&#180;-phosphate or a 5&#180;-OH end.
To map and quantitate ribonucleotides in genomic DNA, the method combines cleavage by a sequence specific endonuclease and alkaline hydrolysis generating 5&#180;-phosphate ends at sites where the specific recognition sequence for the endonuclease is located and 5&#180;-OH ends at positions where ribonucleotides were located. Since the generated free ends are subsequently ligated with adapters and sequenced using Next-generation sequencing, it is of importance to use highly intact DNA and avoid random fragmentation during DNA extraction and library preparation. Assessing these reads normalized to the reads at the endonuclease cleavage sites allows a simultaneous quantitation and mapping of the detected ribonucleotides. Free 5&#180;-ends are detected in control experiments where the alkaline hydrolysis of DNA is replaced by treatment with KCl. The acquired data provide insight into ribonucleotide location and quantity and allows analyses with respect to ribonucleotide content and incorporation frequency.

<table><tbody><tr><td>10x T4 Polynucleotide Kinase Reaction Buffer</td><td>New England Biolabs</td><td>B0201S</td><td></td></tr><tr><td>10x T4 RNA Ligase Reaction Buffer</td><td>New England Biolabs</td><td>B0216L</td><td></td></tr><tr><td>1x PBS</td><td>Medicago</td><td>09-9400-100</td><td>dissolve 1 tablet in H&lt;sub&gt;2&lt;/sub&gt;O to a final volume of 1 L</td></tr><tr><td>2-Propanol</td><td>Sigma-Aldrich</td><td>33539-1L-GL-R</td><td></td></tr><tr><td>2100 Bioanalyzer</td><td>Agilent Technologies</td><td>G2940CA</td><td></td></tr><tr><td>50 mL Centrifuge Tube</td><td>VWR</td><td>525-0610</td><td></td></tr><tr><td>Adenosine 5&#039;-Triphosphate (ATP, 10 mM)</td><td>New England Biolabs</td><td>P0756S</td><td>dilute with EB to 2 mM</td></tr><tr><td>Agilent DNA 1000 Kit</td><td>Agilent Technologies</td><td>5067-1504</td><td></td></tr><tr><td>BSA, Molecular Biology Grade (20 mg/mL)</td><td>New England Biolabs</td><td>B9000S</td><td>diltue with nuclease-free H&lt;sub&gt;2&lt;/sub&gt;O to 1 mg/mL</td></tr><tr><td>Buffer EB</td><td>QIAGEN</td><td>19086</td><td>referred to as EB</td></tr><tr><td>CleanPCR paramagnetic beads</td><td>CleanNA</td><td>CPCR-0050</td><td></td></tr><tr><td>Deoxynucleotide (dNTP) Solution Mix (10 mM each)</td><td>New England Biolabs</td><td>N0447L</td><td>dilute with EB to 2 mM</td></tr><tr><td>DMEM, high glucose, GlutaMAX Supplement</td><td>Gibco</td><td>61965026</td><td></td></tr><tr><td>DynaMag 96 Side</td><td>Thermo Fisher</td><td>12331D</td><td></td></tr><tr><td>Ethanol 99.5% analytical grade</td><td>Solveco</td><td>1395</td><td>dilute with milliQ water to 70%</td></tr><tr><td>Ethylenediaminetetraacetic acid solution (EDTA, 0.5 M)</td><td>Sigma-Aldrich</td><td>03690-100ML</td><td></td></tr><tr><td>Fetal bovine serum</td><td>Gibco</td><td>10500056</td><td></td></tr><tr><td>HEPES buffer pH 8.0 (1 M) sterile BC</td><td>AppliChem</td><td>A6906,0125</td><td></td></tr><tr><td>Hexammine cobalt(III) chloride (CoCl&lt;sub&gt;3&lt;/sub&gt;(NH&lt;sub&gt;3&lt;/sub&gt;)&lt;sub&gt;6&lt;/sub&gt;)</td><td>Sigma-Aldrich</td><td>H7891-5G</td><td>dissolve in nuclease-free H&lt;sub&gt;2&lt;/sub&gt;O for 10&amp;nbsp;M solution, sterile filter. CAUTION: carcinogenic, sensitizing and hazardous to aquatic environment.</td></tr><tr><td>HincII</td><td>New England Biolabs</td><td>R0103S</td><td>supplied with NEBuffer 3.1</td></tr><tr><td>Hybridiser HB-1D</td><td>Techne</td><td>FHB4DD</td><td></td></tr><tr><td>KAPA HiFi HotStart ReadyMix (2X)</td><td>Kapa Biosystems</td><td>KK2602</td><td></td></tr><tr><td>Lysis buffer</td><td></td><td></td><td>50 mM EDTA, 20 mM HEPES, NaCl 75 mM, Proteinase K (200 &amp;micro;g/mL), 1% SDS</td></tr><tr><td>Micro tube 1.5 mL</td><td>Sarstedt</td><td>72.690.001</td><td></td></tr><tr><td>Microcentrifuge 5424R</td><td>Eppendorf</td><td>5404000014</td><td></td></tr><tr><td>Microcentrifuge MiniStar silverline</td><td>VWR</td><td>521-2844</td><td></td></tr><tr><td>Multiply&amp;nbsp;&amp;micro;StripPro 0.2 mL tube</td><td>Sarstedt</td><td>72.991.992</td><td></td></tr><tr><td>Nuclease-free water</td><td>Ambion</td><td>AM9937</td><td></td></tr><tr><td>Phenol &amp;ndash; chloroform &amp;ndash; isoamyl alcohol (25:24:1)</td><td>Sigma-Aldrich</td><td>77617-500ML</td><td></td></tr><tr><td>Potassium chloride (KCl)</td><td>VWR</td><td>26764.232</td><td>dissolve in nuclease-free H&lt;sub&gt;2&lt;/sub&gt;O for 3&amp;nbsp;M solution, sterile filter</td></tr><tr><td>Potassium hydroxide (KOH)</td><td>VWR</td><td>26668.296</td><td>dissolve in nuclease-free H&lt;sub&gt;2&lt;/sub&gt;O for 3&amp;nbsp;M solution, sterile filter</td></tr><tr><td>Proteinase K</td><td>Ambion</td><td>AM2546</td><td></td></tr><tr><td>Qubit 3.0 Fluorometer</td><td>Invitrogen</td><td>Q33216</td><td></td></tr><tr><td>Qubit Assay Tubes</td><td>Invitrogen</td><td>Q32856</td><td></td></tr><tr><td>Qubit dsDNA BR Assay Kit</td><td>Invitrogen</td><td>Q32850</td><td>CAUTION: Contains flammable and toxic components</td></tr><tr><td>Qubit dsDNA HS Assay Kit</td><td>Invitrogen</td><td>Q32851</td><td>CAUTION: Contains flammable and toxic components</td></tr><tr><td>Refrigerated Centrifuge 4K15</td><td>Sigma Laboratory Centrifuges</td><td>No. 10740</td><td></td></tr><tr><td>SDS Solution, 10%</td><td>Invitrogen</td><td>15553-035</td><td></td></tr><tr><td>Sodium acetate buffer solution, pH 5.2, 3 M (NaAc)</td><td>Sigma-Aldrich</td><td>S7899</td><td></td></tr><tr><td>Sodium chloride (NaCl)</td><td>VWR</td><td>27810.295</td><td>dissolve in nuclease-free H&lt;sub&gt;2&lt;/sub&gt;O for 5&amp;nbsp;M solution, sterile filter</td></tr><tr><td>T100 Thermal Cycler</td><td>Bio-Rad</td><td>1861096</td><td></td></tr><tr><td>T4 Polynucleotide Kinase (3&#039; phosphatase minus)</td><td>New England Biolabs</td><td>M0236L</td><td></td></tr><tr><td>T4 RNA Ligase 1 (ssRNA Ligase)</td><td>New England Biolabs</td><td>M0204L</td><td>supplied with PEG 8000 (50%)</td></tr><tr><td>T7 DNA Polymerase (unmodified)</td><td>New England Biolabs</td><td>M0274S</td><td>supplied with 10x T7 DNA Polymerase Reaction Buffer</td></tr><tr><td>TE Buffer</td><td>Invitrogen</td><td>12090015</td><td></td></tr><tr><td>ThermoMixer F2.0</td><td>Eppendorf</td><td>5387000013</td><td></td></tr></tbody></table>

simultaneous mapping and quantitation of ribonucleotides in human mitochondrial dna

Established approaches to estimate the number of ribonucleotides present in a genome are limited to the quantitation of incorporated ribonucleotides using short synthetic DNA fragments or plasmids as templates and then extrapolating the results to the whole genome. Alternatively, the number of ribonucleotides present in a genome may be estimated using alkaline gels or Southern blots. More recent in vivo approaches employ Next-generation sequencing allowing genome-wide mapping of ribonucleotides, providing the position and identity of embedded ribonucleotides. However, they do not allow quantitation of the number of ribonucleotides which are incorporated into a genome. Here we describe how to simultaneously map and quantitate the number of ribonucleotides which are incorporated into human mitochondrial DNA in vivo by Next-generation sequencing. We use highly intact DNA and introduce sequence specific double strand breaks by digesting it with an endonuclease, subsequently hydrolyzing incorporated ribonucleotides with alkali. The generated ends are ligated with adapters and these ends are sequenced on a Next-generation sequencing machine. The absolute number of ribonucleotides can be calculated as the number of reads outside the recognition site per average number of reads at the recognition site for the sequence specific endonuclease. This protocol may also be utilized to map and quantitate free nicks in DNA and allows adaption to map other DNA lesions that can be processed to 5&#180;-OH ends or 5&#180;-phosphate ends. Furthermore, this method can be applied to any organism, given that a suitable reference genome is available. This protocol therefore provides an important tool to study DNA replication, 5&#180;-end processing, DNA damage, and DNA repair.

Illustrating the methodology described above, representative data were generated analyzing human mitochondrial DNA from HeLa cells12. Figure 2B shows the summarized reads at all HincII sites in heavy (HS) and light strand (LS) of human mtDNA after KCl treatment (left panels). Around 70% of all detected 5&#180;-ends localize to the cut-sites, demonstrating the high efficiency of the HincII digestion. Treating libraries with KOH to hydrolyze the DNA at embedded ribonucleotides decreases the number of reads at HincII sites to about 40% (Figure 2B, right panels). This is expected since large numbers of 5&#180;-ends are generated at the sites of ribonucleotide incorporation, and is indicative of a sufficient library quality. Figure 2C illustrates the localization and frequency of 5&#180;-ends (green) after KCl treatment and reads generated by HydEn-seq (magenta) after KOH treatment, detecting both free 5&#180;-ends and ends generated at ribonucleotides by alkaline hydrolysis. Free 5&#180;-ends and ribonucleotides localizing to the HS of human mtDNA are shown in the left panel and those localizing to the LS are shown in the right panel. The relative numbers of raw reads at ribonucleotides (Figure 2D, upper panel) or HincII sites (lower panel) on HS and LS of mtDNA show, respectively, a 14-fold or 31-fold stronger coverage of the LS relative to the HS, while a similar bias was not observed for nuclear DNA. This strand bias may be explained by the distinct difference in base composition of the two strands and illustrates the importance of the normalization to reads at HincII sites.
Normalizing read counts to HincII gives a quantitative measure of the number of ribonucleotides per mitochondrial genome (Figure 3A). As illustrated in Figure 3B, the reads after KOH treatment for each ribonucleotide normalized to the sequence composition of each strand show a ratio different than 1, indicating a non-random distribution of reads suggesting a distinct ribonucleotide pattern and a high library quality. That ratio is unaffected by previous digestion with HincII, verifying the enzyme&#39;s cleavage specificity. Normalizing the reads at the sites of embedded ribonucleotides to those at HincII cleavage sites, as well as to the genome nucleotide content, generates a quantitative measure of how many of each ribonucleotide are incorporated per 1,000 complementary bases (Figure 3C).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/56551/56551fig1.jpg" /> 
Figure 1: Schematic for DNA Processing and Library Preparation. (1) Whole genomic DNA is cleaved by HincII for normalization in the subsequent quantitation of ribonucleotides, generating blunt ends at HincII sites (black arrowhead). (2) The DNA is treated with KOH to hydrolyze at ribonucleotide sites, leading to 2&#180;,3&#180;-cyclic phosphate (red pentagon) at 3&#180;-ends and free 5&#180;-OH ends. (3) 5&#180;-OH ends are phosphorylated by T4 Polynucleotide Kinase 3&#180;-phosphatase-minus. (4) All 5&#180;-ends carrying a phosphate group are ligated to the ARC140 oligonucleotide by T4 RNA ligase. (5) The second strand is synthesized using T7 DNA Polymerase and the ARC76-77 oligonucleotides containing random N6 sequences. (6) The library is amplified by a high-fidelity DNA Polymerase using ARC49 and one of the ARC78 to ARC107 index primers containing a unique barcode for multiplexing. (7) 5&#180;-ends are located by paired-end sequencing. <a href="https://cloudflare.jove.com/files/ftp_upload/56551/56551fig1large.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/56551/56551fig2.jpg" /> 
Figure 2: Method validation. (A) Representative electropherograms generated using an automated electrophoresis system to determine the quality of generated libraries treated with KOH or KCl. (B) Summarized signal at HincII sites in heavy (HS) and light strand (LS) human mtDNA after KCl (left panels) or KOH (right panels) treatment. (C) Circos figure of free 5&#180;-ends (green) and from HydEn-Seq (free 5&#180;-ends and ribonucleotides, magenta) in HS (left panel) and LS (right panel) human mtDNA. Peaks are normalized to per million reads and the maximum peak is adjusted to the maximum number of reads of the HydEn-seq library. (D) Summarized raw reads at ribonucleotides (upper panel) and HincII sites (lower panel) in heavy (H) and light (L) strand in human mtDNA (Mito.) or in reverse (RV) or forward (FW) strand in nuclear (Nuc.) DNA. Figures B, C and D are adapted from reference12. Error bars represent the standard error of the mean. <a href="https://cloudflare.jove.com/files/ftp_upload/56551/56551fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/56551/56551fig3.jpg" /> 
Figure 3: Representative Results. (A) The relative number of ribonucleotides normalized to reads at HincII sites for KOH treated libraries on the heavy (H) or light (L) strand. (B) Ratio of ribonucleotide identity to mtDNA genome composition for KOH treated (KOH) and HincII cleaved with KOH treated (HincII+KOH) libraries on the heavy (H) or light (L) strand of mtDNA. (C) Ribonucleotide frequency normalized to 1,000 complementary bases for HincII and KOH treated libraries on the heavy (H) or light (L) strand of mtDNA. Figures are adapted from reference12. Error bars represent the standard error of the mean. <a href="https://cloudflare.jove.com/files/ftp_upload/56551/56551fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td>Name</td>
			<td colspan="4">Sequence</td>
		</tr>
		<tr>
			<td>ARC49</td>
			<td colspan="4">AATGATACGGCGACCACCGAGATCTACACTCTTTCCCTACACGACGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC76</td>
			<td colspan="4">GTGACTGGAGTTCAGACGTGTGCTCTTCCGATCTNNNN*N*N</td>
		</tr>
		<tr>
			<td>ARC77</td>
			<td colspan="4">AGATCGGAAGAGCACACGTCTGAACTCCAGTC*A*C</td>
		</tr>
		<tr>
			<td>ARC78</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATCGTGATGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC84</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATACATCGGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC85</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATGCCTAAGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC86</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATTGGTCAGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC87</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATCACTGTGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC88</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATATTGGCGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC89</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATGATCTGGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC90</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATTCAAGTGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC91</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATCTGATCGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC93</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATAAGCTAGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC94</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATGTAGCCGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC95</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATTACAAGGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC96</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATTGTTGACTGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC97</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATACGGAACTGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC98</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATTCTGACATGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC99</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATCGGGACGGGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC100</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATGTGCGGACGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC101</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATCGTTTCACGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC102</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATAAGGCCACGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC103</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATTCCGAAACGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC104</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATTACGTACGGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC105</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATATCCACTCGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC106</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATATATCAGTGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC107</td>
			<td colspan="4">CAAGCAGAAGACGGCATACGAGATAAAGGAATGTGACTGGAGTTCAGACGTGTGCTCTTCCGATCT</td>
		</tr>
		<tr>
			<td>ARC140</td>
			<td colspan="4">/5AmMC6/ACACTCTTTCCCTACACGACGCTCTTCCGATCT</td>
		</tr>
	</tbody>
</table>
Table 1: Oligonucleotides. Listed are the oligonucleotides used for HydEn-Seq. Bold face indicates indexing. * indicates a phosphorothioate bond. ARC140 contains a 5&#180;-amino group instead of a 5&#180;-OH group, in combination with a C6 linker. This modification reduces formation of ARC140 concatemers during ligation.

Watch this Scientific Journal Video about Simultaneous Mapping and Quantitation of Ribonucleotides in Human Mitochondrial DNA at JoVE.com

Simultaneous Mapping and Quantitation of Ribonucleotides in Human Mitochondrial DNA

Here we describe a method amenable to simultaneously quantitate and genome-wide map ribonucleotides in highly intact DNA at single-nucleotide resolution, combining enzymatic cleavage of genomic DNA with its alkaline hydrolysis and subsequent 5&#180;-end sequencing.

Established approaches to estimate the number of ribonucleotides present in a genome are limited to the quantitation of incorporated ribonucleotides using ...

simultaneous-mapping-quantitation-ribonucleotides-human-mitochondrial

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Biology

9.4K Views.  University of Gothenburg. Hier beschrijven we een methode die zich lenen voor het gelijktijdig kwantificeren en genoom-brede kaart ribonucleotides in zeer intact DNA op single-nucleotide de resolutie, enzymatische splitsing van genomic DNA te combineren met de alkalische hydrolyse en de daaropvolgende 5´-end sequencing.

Video: Simultaneous Mapping and Quantitation of Ribonucleotides in Human Mitochondrial DNA

Visualization of Mitochondrial DNA Replication in Individual Cells by EdU Signal Amplification

Mitochondria are key regulators of cellular energy and mitochondrial biogenesis is an essential component of regulating mitochondria numbers in healthy cells1-3. One approach for monitoring mitochondrial biogenesis is to measure the rate of mitochondrial DNA (mtDNA) replication4. We developed a sensitive technique to label newly synthesized mtDNA in individual cells in order to study mtDNA biogenesis. The technique combines the incorporation of 5-ethynyl-2'-deoxyuridine (EdU)5-7 with a tyramide signal amplification (TSA)8 protocol to visualize mtDNA replication within subcellular compartments of neurons. EdU is superior to other thymidine analogs, such as 5-bromo-2-deoxyuridine (BrdU), because the initial click reaction to label EdU5-7 does not require the harsh acid treatments or enzyme digests that are required for exposing the BrdU epitope. The milder labeling of EdU allows for direct comparison of its incorporation with other cellular markers9-10. The ability to visualize and quantify mtDNA biogenesis provides an essential tool for investigating the mechanisms used to regulate mitochondrial biogenesis and would provide insight into the pathogenesis associated with drug toxicity, aging, cancer and neurodegenerative diseases. Our technique is applicable to sensory neurons as well as other cell types. The use of this technique to measure mtDNA biogenesis has significant implications in furthering the understanding of both normal cellular physiology as well as impaired disease states.

We developed a sensitive technique to label newly synthesized mitochondrial DNA (mtDNA) in individual cells in order to study mtDNA biogenesis. The technique combines the incorporation of EdU together with a tyramide signal amplification (TSA) protocol to visualize mtDNA replication within subcellular compartments of neurons.

Mitochondria are key regulators of cellular energy and mitochondrial biogenesis is an essential component of regulating mitochondria numbers in healthy ...

Neuroscience

Methodology for Accurate Detection of Mitochondrial DNA Methylation

Quantification of DNA methylation can be achieved using bisulfite sequencing, which takes advantage of the property of sodium bisulfite to convert unmethylated cytosine into uracil, in a single-stranded DNA context. Bisulfite sequencing can be targeted (using PCR) or performed on the whole genome and provides absolute quantification of cytosine methylation at the single base-resolution. Given the distinct nature of nuclear- and mitochondrial DNA, notably in the secondary structure, adaptions of bisulfite sequencing methods for investigating cytosine methylation in mtDNA should be made. Secondary and tertiary structure of mtDNA can indeed lead to bisulfite sequencing artifacts leading to false-positives due to incomplete denaturation poor access of bisulfite to single-stranded DNA. Here, we describe a protocol using an enzymatic digestion of DNA with BamHI coupled with bioinformatic analysis pipeline to allow accurate quantification of cytosine methylation levels in mtDNA. In addition, we provide guidelines for designing the bisulfite sequencing primers specific to mtDNA, in order to avoid targeting undesirable NUclear MiTochondrial segments (NUMTs) inserted into the nuclear genome.

Here, we present a protocol to allow accurate quantification of mitochondrial DNA (mtDNA) methylation. In this protocol, we describe an enzymatic digestion of DNA with BamHI coupled with a bioinformatic analysis pipeline which can be used to avoid overestimation of mtDNA methylation levels caused by the secondary structure of mtDNA.

Quantification of DNA methylation can be achieved using bisulfite sequencing, which takes advantage of the property of sodium bisulfite to convert ...

Genetics

Probing for Mitochondrial Complex Activity in Human Embryonic Stem Cells

Mitochondria are cytoplasmic organelles that have a primary role in cellular metabolism and homeostasis, regulation of the cell signaling network, and programmed cell death. Mitochondria produce ATP, regulate the cytoplasmic redox state and Ca2+ balance, catabolize fatty acids, synthesize heme, nucleotides, steroid hormones, amino acids, and help assemble iron-sulfur clusters in proteins. Mitochondria also have an essential role in heat production. Mutations of the mitochondrial genome cause several types of human disorder. The accumulation of mtDNA mutations correlates with aging and is suspected to have an important role in the development of cancer. Due to their vitally important role in all cell types, the function of mitochondria must also be critical for stem cells. Key advances have been made in our understanding of stem cell viability, proliferation, and differentiation capacity. But the functional activity of stem cells, in particular their energy status, was not yet been studied in detail. Almost nothing is known about the mitochondrial properties of human embryonic stem cells (hESCs) and their differentiated precursor progeny. One way to understand and evaluate the role of mitochondria in hESC function and developmental potential is to directly measure the activity of mitochondrial respiratory complexes. Here, we describe high resolution clear native gel electrophoresis and subsequent in gel activity visualization as a method for analyzing the five respiratory chain complexes of hESCs.

In this video, we will show you how the mitochondrial respiratory chain complexes of human embryonic stem cells can be analyzed using in gel activity assays.

Mitochondria are cytoplasmic organelles that have a primary role in cellular metabolism and homeostasis, regulation of the cell signaling network, and ...

Discrimintion and Mapping of the Primary and Processed Transcripts in Maize Mitochondrion Using a Circular RT-PCR-based Strategy

In plant mitochondria, some steady-state transcripts have 5&#39; triphosphate derived from transcription initiation (primary transcripts), while the others contain 5&#39; monophosphate generated post-transcriptionally (processed transcripts). To discriminate between the two types of transcripts, several strategies have been developed, and most of them depend on presence/absence of 5&#39; triphosphate. However, the triphosphate at primary 5&#39; termini is unstable, and it hinders a clear discrimination of the two types of transcripts. To systematically differentiate and map the primary and processed transcripts stably accumulated in maize mitochondrion, we have developed a circular RT-PCR (cRT-PCR)-based strategy by combining cRT-PCR, RNA 5&#39; polyphoshpatase treatment, quantitative RT-PCR (RT-qPCR), and Northern blot. As an improvement, this strategy includes an RNA normalization step to minimize the influence of unstable 5&#39; triphosphate.
In this protocol, the enriched mitochondrial RNA is pre-treated by RNA 5&#39; polyphosphatase, which converts 5&#39; triphsophate to monophosphate. After circularization and reverse transcription, the two cDNAs derived from 5&#39; polyphosphatase-treated and non-treated RNAs are normalized by maize 26S mature rRNA, which has a processed 5&#39; end and is insensitive to 5&#39; polyphosphatase. After normalization, the primary and processed transcripts are discriminated by comparing cRT-PCR and RT-qPCR products obtained from the treated and non-treated RNAs. The transcript termini are determined by cloning and sequencing of the cRT-PCR products, and then verified by Northern blot.
By using this strategy, most steady-state transcripts in maize mitochondrion have been determined. Due to the complicated transcript pattern of some mitochondrial genes, a few steady-state transcripts were not differentiated and/or mapped, though they were detected in a Northern blot. We are not sure whether this strategy is suitable to discriminate and map the steady-state transcripts in other plant mitochondria or in plastids.

We present a circular RT-PCR-based strategy by combining circular RT-PCR, quantitative RT-PCR, RNA 5&#39; polyphosphatase-treatment, and Northern blot. This protocol includes a normalization step to minimize the influence of unstable 5&#39; triphosphate, and it is suitable for discriminating and mapping the primary and processed transcripts stably accumulated in maize mitochondrion.

In plant mitochondria, some steady-state transcripts have 5&#39; triphosphate derived from transcription initiation (primary transcripts), while the ...

A Rapid High-throughput Method for Mapping Ribonucleoproteins (RNPs) on Human pre-mRNA

Sequencing RNAs that co-immunoprecipitate (co-IP) with RNA binding proteins has increased our understanding of splicing by demonstrating that binding location often influences function of a splicing factor.  However, as with any sampling strategy the chance of identifying an RNA bound to a splicing factor is proportional to its cellular abundance.  We have developed a novel in vitro approach for surveying binding specificity on otherwise transient pre-mRNA. This approach utilizes a specifically designed oligonucleotide pool that tiles across introns, exons, splice junctions, or other pre-mRNA.  The pool is subjected to some kind of molecular selection. Here, we demonstrate the method by separating the oligonucleotide into a bound and unbound fraction and utilize a two color array strategy to record the enrichment of each oligonucleotide in the bound fraction. The array data generates high-resolution maps with the ability to identify sequence-specific and structural determinates of ribonucleoprotein (RNP) binding on pre-mRNA.  A unique advantage to this method is its ability to avoid the sampling bias towards mRNA associated with current IP and SELEX techniques, as the pool is specifically designed and synthesized from pre-mRNA sequence. The flexibility of the oligonucleotide pool is another advantage since the experimenter chooses which regions to study and tile across, tailoring the pool to their individual needs.  Using this technique, one can assay the effects of polymorphisms or mutations on binding on a large scale or clone the library into a functional splicing reporter and identify oligonucleotides that are enriched in the included fraction.  This novel in vitro high-resolution mapping scheme provides a unique way to study RNP interactions with transient pre-mRNA species, whose low abundance makes them difficult to study with current in vivo techniques.  



A Rapid High-throughput Method for Mapping Ribonucleoproteins RNPs on Human pre-mRNA

Due to the transient nature of pre-mRNA, it can be difficult to isolate and study in vivo. Here, we present a novel in vitro approach to investigate RNA-protein interactions using a synthetic oligo pool that tiles across selected regions of pre-mRNA.

Sequencing RNAs that co-immunoprecipitate (co-IP) with RNA binding proteins has increased our understanding of splicing by demonstrating that binding ...

Fate Mapping of Human Embryonic Stem Cells by Teratoma Formation 

Human embryonic stem cells (hESCs) have an unlimited capacity for self-renewal, and the ability to differentiate into cells derived from all three embryonic germ layers (1). Directed differentiation of hESCs into specific cell types has generated much interest in the field of regenerative medicine (e.g., (2-5)), and methods for determining the in vivo fate of selected or manipulated hESCs are essential to this endeavor. We have adapted a highly efficient teratoma formation assay for this purpose. A small number of specifically selected hESCs is mixed with undifferentiated wild type hESCs and Phaseolus vulgaris lectin to form a cell pellet. This is grafted beneath the kidney capsule in an immunodeficient mouse. As few as 2.5 x 105 hESCs are needed to form a 16 cm3 teratoma within 8-12 weeks. The fate of the originally selected hESCs can then be determined by immunohistochemistry. This method provides a valuable tool for characterizing tissue-specific reagents for cell-based therapy.

Fate Mapping of Human Embryonic Stem Cells by Teratoma Formation

Directed differentiation of hESCs into specific cells has generated much interest in regenerative medicine. We provide a concise, step-by-step protocol for determining the in vivo fate of selected hESCs that provides a valuable tool for characterizing tissue-specific reagents for cell-based therapy.

Human embryonic stem cells (hESCs) have an unlimited capacity for self-renewal, and the ability to differentiate into cells derived from all three ...

High-Throughput Quantification of the Synthesis and Distribution of mtDNA

High-Throughput Image-Based Quantification of Mitochondrial DNA Synthesis and Distribution

The vast majority of cellular processes require a continuous supply of energy, the most common carrier of which is the ATP molecule. Eukaryotic cells produce most of their ATP in the mitochondria by oxidative phosphorylation. Mitochondria are unique organelles because they have their own genome that is replicated and passed on to the next generation of cells. In contrast to the nuclear genome, there are multiple copies of the mitochondrial genome in the cell. The detailed study of the mechanisms responsible for the replication, repair, and maintenance of the mitochondrial genome is essential for understanding the proper functioning of mitochondria and whole cells under both normal and disease conditions. Here, a method that allows the high-throughput quantification of the synthesis and distribution of mitochondrial DNA (mtDNA) in human cells cultured in vitro is presented. This approach is based on the immunofluorescence detection of actively synthesized DNA molecules labeled by 5-bromo-2'-deoxyuridine (BrdU) incorporation and the concurrent detection of all the mtDNA molecules with anti-DNA antibodies. Additionally, the mitochondria are visualized with specific dyes or antibodies. The culturing of cells in a multi-well format and the utilization of an automated fluorescence microscope make it easier to study the dynamics of mtDNA and the morphology of mitochondria under a variety of experimental conditions in a relatively short time.

Author Spotlight: High-Throughput Image-Based Quantification of Mitochondrial DNA Synthesis and Distribution  

A procedure for studying the dynamics of mitochondrial DNA (mtDNA) metabolism in cells using a multi-well plate format and automated immunofluorescence imaging to detect and quantify mtDNA synthesis and distribution is described. This can be further used to investigate the effects of various inhibitors, cellular stresses, and gene silencing on mtDNA metabolism.

The vast majority of cellular processes require a continuous supply of energy, the most common carrier of which is the ATP molecule. Eukaryotic cells ...

Biochemistry

Simultaneous Measurement of Mitochondrial Calcium and Mitochondrial Membrane Potential in Live Cells by Fluorescent Microscopy

Apart from their essential role in generating ATP, mitochondria also act as local calcium (Ca2+) buffers to tightly regulate intracellular Ca2+ concentration. To do this, mitochondria utilize the electrochemical potential across their inner membrane (&#916;&#936;m) to sequester Ca2+. The influx of Ca2+ into the mitochondria stimulates three rate-limiting dehydrogenases of the citric acid cycle, increasing electron transfer through the oxidative phosphorylation (OXPHOS) complexes. This stimulation maintains &#916;&#936;m, which is temporarily dissipated as the positive calcium ions cross the mitochondrial inner membrane into the mitochondrial matrix.
We describe here a method for simultaneously measuring mitochondria Ca2+ uptake and &#916;&#936;m in live cells using confocal microscopy. By permeabilizing the cells, mitochondrial Ca2+ can be measured using the fluorescent Ca2+ indicator Fluo-4, AM, with measurement of &#916;&#936;m using the fluorescent dye tetramethylrhodamine, methyl ester, perchlorate (TMRM). The benefit of this system is that there is very little spectral overlap between the fluorescent dyes, allowing accurate measurement of mitochondrial Ca2+ and &#916;&#936;m simultaneously. Using the sequential addition of Ca2+ aliquots, mitochondrial Ca2+ uptake can be monitored, and the concentration at which Ca2+ induces mitochondrial membrane permeability transition and the loss of &#916;&#936;m determined.

Mitochondria can utilize the electrochemical potential across their inner membrane (&#916;&#936;m) to sequester calcium (Ca2+), allowing them to shape cytosolic Ca2+ signaling within the cell. We describe a method for simultaneously measuring mitochondria Ca2+ uptake and &#916;&#936;m in live cells using fluorescent dyes and confocal microscopy.

Apart from their essential role in generating ATP, mitochondria also act as local calcium (Ca2+) buffers to tightly regulate intracellular Ca2+ ...

Genotyping Single Nucleotide Polymorphisms in the Mitochondrial Genome by Pyrosequencing

Mutations in the mitochondrial genome (mtDNA) have been associated with maternally inherited genetic diseases. However, interest in mtDNA polymorphisms has increased in recent years due to the recently developed ability to produce models by mtDNA mutagenesis and a new appreciation of the association between mitochondrial genetic aberrations and common age-related diseases such as cancer, diabetes, and dementia. Pyrosequencing is a sequencing-by-synthesis technique that is widely employed across the mitochondrial field for routine genotyping experiments. Its relative affordability when compared to massive parallel sequencing methods and ease of implementation make it an invaluable technique in the field of mitochondrial genetics, allowing for the rapid quantification of heteroplasmy with increased flexibility. Despite the practicality of this method, its implementation as a means of mtDNA genotyping requires the observation of certain guidelines, specifically to avoid certain biases of biological or technical origin. This protocol outlines the necessary steps and precautions in designing and implementing pyrosequencing assays for use in the context of heteroplasmy measurement.

Pyrosequencing assays enable the robust and rapid genotyping of mitochondrial DNA single nucleotide polymorphisms in heteroplasmic cells or tissues.

Mutations in the mitochondrial genome (mtDNA) have been associated with maternally inherited genetic diseases. However, interest in mtDNA polymorphisms ...

Medicine

Specific Labeling of Mitochondrial Nucleoids for Time-lapse Structured Illumination Microscopy

Mitochondrial nucleoids are compact particles formed by mitochondrial DNA molecules coated with proteins. Mitochondrial DNA encodes tRNAs, rRNAs, and several essential mitochondrial polypeptides. Mitochondrial nucleoids divide and distribute within the dynamic mitochondrial network that undergoes fission/fusion and other morphological changes. High resolution live fluorescence microscopy is a straightforward technique to characterize a nucleoid&#39;s position and motion. For this technique, nucleoids are commonly labeled through fluorescent tags of their protein components, namely transcription factor a (TFAM). However, this strategy needs overexpression of a fluorescent protein-tagged construct, which may cause artifacts (reported for TFAM), and is not feasible in many cases. Organic DNA-binding dyes do not have these disadvantages. However, they always show staining of both nuclear and mitochondrial DNAs, thus lacking specificity to mitochondrial nucleoids. By taking into account the physico-chemical properties of such dyes, we selected a nucleic acid gel stain (SYBR Gold) and achieved preferential labeling of mitochondrial nucleoids in live cells. Properties of the dye, particularly its high brightness upon binding to DNA, permit subsequent quantification of mitochondrial nucleoid motion using time series of super-resolution structured illumination images.

The protocol describes specific labeling of mitochondrial nucleoids with a commercially available DNA gel stain, acquisition of time lapse series of live labeled cells by super-resolution structured illumination microscopy (SR-SIM), and automatic tracking of nucleoid motion.

Mitochondrial nucleoids are compact particles formed by mitochondrial DNA molecules coated with proteins. Mitochondrial DNA encodes tRNAs, rRNAs, and ...

Simultaneous Mapping and Quantitation of Ribonucleotides in Human Mitochondrial DNA

Samenvatting

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