Ligation sequencing gDNA - sequence capture (SQK-LSK110)

Version for device: MinION

1. Important This is a Legacy product

   This kit is soon to be discontinued and we recommend all customers to upgrade to the latest chemistry for their relevant kit which is available on the Store. If customers require further support for any ongoing critical experiments using a Legacy product, please contact Customer Support via email: support@nanoporetech.com. For further information on please see the product update page.

2. Sequence capture protocol features

   Use this protocol if you:

   • Are not interested in analysing the entire genome
   • Want greater depth of coverage of a specific region
   • Want to analyse a large number of target regions
3. Introduction to sequence capture

   This protocol describes how to carry out sequence capture of genomic DNA using the Ligation Sequencing Kit (SQK-LSK110) and the Agilent SureSelect method for the kit used (e.g. SureSelect Human All Exon). Other kits of exome probes are available depending on the exome region coverage required.

   Steps in the sequencing workflow:

   Prepare for your experiment

   You will need to:
   - Ensure you have your sequencing kit, the correct equipment and third-party reagents
   - Download the software for acquiring and analysing your data
   - Check your flow cell to ensure it has enough pores for a good sequencing run

   Library preparation

   You will need to:
   - Fragment your DNA (this step is optional)
   - Ligate PCR adapters to the DNA ends and amplify the fragments
   - Hybridise the DNA to probes provided in the Agilent SureSelect Exome kit, and perform a pulldown
   - Elute and amplify the pulled-down fragments
   - Prepare the DNA ends for adapter attachment
   - Attach sequencing adapters supplied in the kit to the DNA ends
   - Prime the flow cell, and load your DNA library into the flow cell

   

   Sequencing and analysis

   You will need to:
   - Start a sequencing run using the MinKNOW software, which will collect raw data from the device and convert it into basecalled reads
   - Start the EPI2ME software and select a workflow for Human Exome mapping

4. We recommend using the standard SureSelect Target Enrichment System protocol from Agilent Technologies with the following differences:
   • The DNA in this protocol is sheared with dsDNA Fragmentase rather than in a Covaris microTUBE, and is incubated at 16° C instead of the 37° C recommended by NEB
   • DNA purification in this protocol is carried out using Agencourt AMPure XP beads instead of QIAquick PCR purification
   • DNA End-prep is carried out using the NEBNext Ultra II End Repair/dA-Tailing Module instead of the Agilent method
   • Ligation of PCR adapters is carried out using the NEB Blunt/TA Ligase Master Mix instead of the Agilent method
   • No desalting of the capture solution is necessary
   • Long AMP Taq is used for amplification of the DNA post-hybridisation
5. Important This protocol is for the preparation of a single sample. Multiple samples can be prepared in parallel; each sample will require a separate pull-down and will need to be run on a separate flow cell.
6. Important Compatibility of this protocol

   This protocol should only be used in combination with:

   • Ligation Sequencing Kit (SQK-LSK110)
   • Control Expansion (EXP-CTL001)
   • PCR Expansion (EXP-PCA001)
   • FLO-MIN106 (R9.4.1) flow cells
   • Flow Cell Wash Kit (EXP-WSH004)

1. For this protocol, you will need 3.5 µg high molecular weight human genomic DNA.
2. Input DNA

   How to QC your input DNA

   It is important that the input DNA meets the quantity and quality requirements. Using too little or too much DNA, or DNA of poor quality (e.g. highly fragmented or containing RNA or chemical contaminants) can affect your library preparation.

   For instructions on how to perform quality control of your DNA sample, please read the Input DNA/RNA QC protocol.

   Chemical contaminants

   Depending on how the DNA is extracted from the raw sample, certain chemical contaminants may remain in the purified DNA, which can affect library preparation efficiency and sequencing quality. Read more about contaminants on the Contaminants page of the Community.

3. NEBNext® Companion Module for Oxford Nanopore Technologies® Ligation Sequencing

   For customers new to nanopore sequencing, we recommend buying the NEBNext® Companion Module for Oxford Nanopore Technologies® Ligation Sequencing (catalogue number E7180S or E7180L), which contains all the NEB reagents needed for use with the Ligation Sequencing Kit.

   Please note, for our amplicon protocols, NEBNext FFPE DNA Repair Mix and NEBNext FFPE DNA Repair Buffer are not required.

4. Ligation Sequencing Kit (SQK-LSK110) contents

   

   Name	Acronym	Cap colour	No. of vials	Fill volume per vial (µl)
   DNA CS	DCS	Yellow	1	35
   Adapter Mix F	AMX-F	Green	1	40
   Ligation Buffer	LNB	Clear	1	200
   L Fragment Buffer	LFB	White cap, orange stripe on label	2	1,800
   S Fragment Buffer	SFB	Grey	2	1,800
   Sequencing Buffer II	SBII	Red	1	500
   Elution Buffer	EB	Black	1	200
   Loading Beads II	LBII	Pink	1	360
   Loading Solution	LS	White cap, pink sticker on label	1	360
   Flush Buffer	FB	Blue	6	1,170
   Flush Tether	FLT	Purple	1	200

1. MinION Mk1B IT requirements

   Sequencing on a MinION Mk1B requires a high-spec computer or laptop to keep up with the rate of data acquisition. Read more in the MinION Mk1B IT Requirements document.

2. MinION Mk1C IT requirements

   The MinION Mk1C contains fully-integrated compute and screen, removing the need for any accessories to generate and analyse nanopore data. Read more in the MinION Mk1C IT requirements document.

3. Software for nanopore sequencing

   MinKNOW

   The MinKNOW software controls the nanopore sequencing device, collects sequencing data and basecalls in real time. You will be using MinKNOW for every sequencing experiment to sequence, basecall and demultiplex if your samples were barcoded.

   For instructions on how to run the MinKNOW software, please refer to the MinKNOW protocol.

   EPI2ME (optional)

   The EPI2ME cloud-based platform performs further analysis of basecalled data, for example alignment to the Lambda genome, barcoding, or taxonomic classification. You will use the EPI2ME platform only if you would like further analysis of your data post-basecalling.

   For instructions on how to create an EPI2ME account and install the EPI2ME Desktop Agent, please refer to the EPI2ME Platform protocol.

4. Check your flow cell

   We highly recommend that you check the number of pores in your flow cell prior to starting a sequencing experiment. This should be done within 12 weeks of purchasing for MinION/GridION/PromethION or within four weeks of purchasing Flongle Flow Cells. Oxford Nanopore Technologies will replace any flow cell with fewer than the number of pores in the table below, when the result is reported within two days of performing the flow cell check, and when the storage recommendations have been followed. To do the flow cell check, please follow the instructions in the Flow Cell Check document.

   Flow cell	Minimum number of active pores covered by warranty
   Flongle Flow Cell	50
   MinION/GridION Flow Cell	800
   PromethION Flow Cell	5000

1. Prepare the DNA in nuclease-free water.
   • Transfer 3.5 μg genomic DNA into a DNA LoBind tube
   • Adjust the volume to 16 μl or less with nuclease-free water
   • Mix thoroughly by inversion avoiding unwanted shearing
   • Spin down briefly in a microfuge

2. Fragment DNA to ~1-2 kb as follows:

   Mix the reagents in the order given below:

   Reagent	Volume
   DNA (1-16 µl)	x µl
   10x Fragmentase Reaction Buffer v2	2 µl
   Nuclease-free water	16 - x µl
   dsDNA Fragmentase	2 µl
   Total	20 µl

3. Vortex for 3 sec.
4. Incubate the reaction for 10 minutes at 16° C.
5. Resuspend the AMPure XP beads by vortexing.
6. Add 36 µl of the AMPure XP beads to the reaction and mix gently by pipetting.
7. Incubate on a Hula mixer (rotator mixer) for 5 minutes at room temperature.
8. Prepare 500 μl of fresh 70% ethanol in nuclease-free water.
9. Spin down the sample and pellet on a magnet. Keep the tube on the magnet, and pipette off the supernatant when clear and colourless.
10. Keep the tube on the magnet and wash the beads with 200 µl of freshly prepared 70% ethanol without disturbing the pellet. Remove the ethanol using a pipette and discard.
11. Spin down and place the tube back on the magnet. Pipette off any residual ethanol. Allow to dry for ~30 seconds, but do not dry the pellet to the point of cracking.
12. Remove the tube from the magnetic rack and resuspend pellet in 48 µl nuclease-free water. Incubate for 2 minutes at room temperature.
13. Pellet the beads on a magnet until the eluate is clear and colourless.
14. Remove and retain 48 µl of eluate into a clean 1.5 ml Eppendorf DNA LoBind tube.
15. Quantify 1 µl of fragmented and repaired DNA using a Qubit fluorometer
16. End of Step 3.5 µg fragmented DNA in 47 µl is taken into the next step.

1. Thaw DNA Control Sample (DCS) at room temperature, spin down, mix by pipetting, and place on ice.
2. Prepare the NEBNext FFPE DNA Repair Mix and NEBNext Ultra II End Repair / dA-tailing Module reagents in accordance with manufacturer’s instructions, and place on ice.

   For optimal performance, NEB recommend the following:

   1. Thaw all reagents on ice.

   2. Flick and/or invert the reagent tubes to ensure they are well mixed.
      
      Note: Do not vortex the FFPE DNA Repair Mix or Ultra II End Prep Enzyme Mix.

   3. Always spin down tubes before opening for the first time each day.

   4. The Ultra II End Prep Buffer and FFPE DNA Repair Buffer may have a little precipitate. Allow the mixture to come to room temperature and pipette the buffer up and down several times to break up the precipitate, followed by vortexing the tube for 30 seconds to solubilise any precipitate.
      
      Note: It is important the buffers are mixed well by vortexing.

   5. The FFPE DNA Repair Buffer may have a yellow tinge and is fine to use if yellow.

3. In a 0.2 ml thin-walled PCR tube, mix the following:

   Between each addition, pipette mix 10-20 times.

   Reagent	Volume
   DNA from the previous step	47 µl
   DNA CS (optional)	1 µl
   NEBNext FFPE DNA Repair Buffer	3.5 µl
   NEBNext FFPE DNA Repair Mix	2 µl
   Ultra II End-prep Reaction Buffer	3.5 µl
   Ultra II End-prep Enzyme Mix	3 µl
   Total	60 µl

4. Ensure the components are thoroughly mixed by pipetting, and spin down.
5. Using a thermal cycler, incubate at 20°C for 5 minutes and 65°C for 5 minutes.
6. Important AMPure XP bead clean-up

   It is recommended that the repaired/end-prepped DNA sample is subjected to the following clean-up with AMPure XP beads. This clean-up can be omitted for simplicity and to reduce library preparation time. However, it has been observed that omission of this clean-up can: reduce subsequent adapter ligation efficiency, increase the prevalence of chimeric reads, and lead to an increase in pores being unavailable for sequencing. If omitting the clean-up step, proceed to the next section.

7. Resuspend the AMPure XP beads by vortexing.
8. Transfer the DNA sample to a clean 1.5 ml Eppendorf DNA LoBind tube.
9. Add 60 µl of resuspended AMPure XP beads to the end-prep reaction and mix by flicking the tube.
10. Incubate on a Hula mixer (rotator mixer) for 5 minutes at room temperature.
11. Prepare 500 μl of fresh 70% ethanol in nuclease-free water.
12. Spin down the sample and pellet on a magnet until supernatant is clear and colourless. Keep the tube on the magnet, and pipette off the supernatant.
13. Keep the tube on the magnet and wash the beads with 200 µl of freshly prepared 70% ethanol without disturbing the pellet. Remove the ethanol using a pipette and discard.
14. Repeat the previous step.
15. Spin down and place the tube back on the magnet. Pipette off any residual ethanol. Allow to dry for ~30 seconds, but do not dry the pellet to the point of cracking.
16. Remove the tube from the magnetic rack and resuspend pellet in 31 µl nuclease-free water. Incubate for 2 minutes at room temperature.
17. Pellet the beads on a magnet until the eluate is clear and colourless, for at least 1 minute.
18. Remove and retain 31 µl of eluate into a clean 1.5 ml Eppendorf DNA LoBind tube.
19. Quantify 1 µl of end-prepped DNA using a Qubit fluorometer - recovery aim > 700 ng.

    

20. End of Step Take forward approximately 700 ng of end-prepped DNA in 30 µl into adapter ligation.

1. Add the reagents in the order given below, mixing by pipetting 10-20 times between each sequential addition:

   Reagent	Volume
   End-prepped DNA	30 µl
   PCR Adapters (PCA)	20 µl
   NEB Blunt/TA Ligase Master Mix	50 µl
   Total	100 µl

2. Mix gently by flicking the tube, and spin down.
3. Incubate the reaction for 10 minutes at room temperature.
4. Resuspend the AMPure XP beads by vortexing.
5. Add 100 µl of resuspended AMPure XP beads to the end-prep reaction and mix by pipetting.

   End-prep cleanup demo

6. Incubate on a Hula mixer (rotator mixer) for 5 minutes at room temperature.
7. Prepare 500 μl of fresh 70% ethanol in nuclease-free water.
8. Spin down the sample and pellet on a magnet. Keep the tube on the magnet, and pipette off the supernatant when clear and colourless.
9. Keep the tube on the magnet and wash the beads with 200 µl of freshly prepared 70% ethanol without disturbing the pellet. Remove the ethanol using a pipette and discard.
10. Repeat the previous step.
11. Spin down and place the tube back on the magnet. Pipette off any residual ethanol. Allow to dry for ~30 seconds, but do not dry the pellet to the point of cracking.
12. Remove the tube from the magnetic rack and resuspend pellet in 49 µl nuclease-free water. Incubate for 2 minutes at room temperature.
13. Pellet the beads on a magnet until the eluate is clear and colourless.
14. Remove and retain 49 µl of eluate into a clean 1.5 ml Eppendorf DNA LoBind tube.
15. Quantify 1 µl of adapted DNA using a Qubit fluorometer.
16. End of Step Take forward 48 µl of the adapted DNA into the PCR reaction. However, at this point it is also possible to store the sample at 4°C overnight.

1. In a 0.2 ml thin-walled PCR tube mix the following:

   Reagent	Volume
   LongAmp Taq 2X Master Mix	50 µl
   PRM Adapters (10 μM)	2 µl
   Template DNA	48 µl
   Total	100 µl

2. Amplify using the following cycling conditions:

   Cycle step	Temperature	Time	No. of cycles
   Initial denaturation	95 °C	3 mins	1
   Denaturation	98 °C	20 secs	6 (b)
   Annealing	62 °C (a)	15 secs (a)	6 (b)
   Extension	65 °C (c)	3 mins	6 (b)
   Final extension	65 °C	3 mins	1
   Hold	4 °C	∞

   a. This is specific to the Oxford Nanopore primer and should be maintained

   b. Adjust accordingly if input quantities are altered

   c. This temperature is determined by the type of polymerase that is being used (given here for LongAmp Taq polymerase)

3. Resuspend the AMPure XP beads by vortexing.
4. Add 40 µl of resuspended AMPure XP beads to the reaction and mix by flicking the tube.
5. Incubate on a Hula mixer (rotator mixer) for 5 minutes at room temperature.
6. Prepare 500 μl of fresh 70% ethanol in nuclease-free water.
7. Spin down the sample and pellet on a magnet. Keep the tube on the magnet, and pipette off the supernatant when clear and colourless.
8. Keep the tube on the magnet and wash the beads with 200 µl of freshly prepared 70% ethanol without disturbing the pellet. Remove the ethanol using a pipette and discard.
9. Repeat the previous step.
10. Spin down and place the tube back on the magnet. Pipette off any residual ethanol. Allow to dry for ~30 seconds, but do not dry the pellet to the point of cracking.
11. Remove the tube from the magnetic rack and resuspend the pellet in 35 µl nuclease-free water. Incubate for 2 minutes at room temperature.
12. Pellet the beads on a magnet until the eluate is clear and colourless.
13. Remove and retain 35 µl of eluate into a clean 1.5 ml Eppendorf DNA LoBind tube.
14. Quantify 2 µl of amplified DNA using a Qubit fluorometer.
15. End of Step Take forward 700–1000 ng amplified DNA into the hybridisation step.

1. In a clean 1.5 ml Eppendorf DNA LoBind tube, mix the following:

   Reagent	Volume
   DNA library	700-1000 ng
   Cot-1 DNA	5 µg
   Blocking oligo top	1 µl

2. The volume of the reaction can be variable, as the water is evaporated in step 2. After this, the DNA is reconstituted to a set volume.
3. Evaporate the water in a SpeedVac at 45ºC for approximately 1 hour.

   Poke one or more holes in the lid with a narrow gauge needle. You can also break off the cap, cover with parafilm, and poke a hole in the parafilm.

4. Reconstitute with nuclease-free water to a final volume of 9 µl. Pipette up and down along the sides of the tube for optimal recovery.
5. Mix thoroughly by vortexing and spin down for 1 minute.
6. Move the 9 µl gDNA library samples to separate wells of a 96-well plate or strip tube. Seal the wells or close the tubes and incubate in the thermal cycler using the following program:

   Stage	Temperature	Time
   Step 1	95 ºC	5 min
   Step 2	65 ºC	5 min
   Step 3	65 ºC	Hold

7. You will now need to prepare the Hybridisation Buffer mix and the RNase Block ready to be combined with the Capture Library reagent from the SureSelect kit. This will then be combined with the adapted, amplified DNA sample.
8. Once the sample tubes are in the thermal cycler, mix the reagents in the table below to make the Hybridisation Buffer:

   Reagent	Volume for 1 reaction
   SureSelect Hyb 1 (orange cap or bottle)	6.63 µl
   SureSelect Hyb 2 (red cap)	0.27 µl
   SureSelect Hyb 3 (yellow cap or bottle)	2.65 µl
   SureSelect Hyb 4 (black cap or bottle)	3.45 µl
   Total	13 µl

   In the event of precipitation, warm the Hybridisation Buffer at 65°C for 5 minutes.
   Otherwise, keep buffer at room temperature until it is used for the Hybridisation mix.

9. Dilute the SureSelect RNase Block (purple cap) in nuclease-free water, sufficient for the number of hybridisation reactions in the run. Keep the mixture on ice.

   Capture library size	RNase block dilution (parts RNase block:water)	Volume of diluted RNase block per hybridisation reaction
   ≥3 Mb	25% (1:3)	2 μl
   <3 Mb	10% (1:9)	5 μl

10. Important Please note that the 1:3 ratio of the RNase Block dilution is different to the SureSelect protocol.
11. Prepare the Capture Library Hybridisation Mix according to the table below. Only keep the mixture at room temperature until it is added to sample wells.

    Reagent	Volume for 1 reaction
    Hybridisation buffer mixture	13 µl
    25% RNase Block solution	2 µl
    Capture library (red cap) ≥3 Mb	5 µl
    Total	20 µl

12. If your capture library is <3 Mb prepare the Capture Library Hybridisation Mix as follows:

    Reagent	Volume for 1 reaction
    Hybridisation buffer mixture	13 µl
    10% RNase Block solution	5 µl
    Capture library (red cap) <3 Mb	2 µl
    Total	20 µl

13. Important Do not keep solutions containing the Capture Library at room temperature for longer than 10 mins.
14. Keeping all reagents at 65°C, add 20 µl of the Capture Hybridisation Mix to each well/tube containing 9 µl adapted and amplified DNA sample.
15. Mix by pipetting.
16. Seal all the wells or replace the caps on the strip tubes.
17. Important Wells must be sealed to minimise evaporation, to avoid a negative impact on your results.
18. Incubate the plate or tubes for 16 to 24 hours at 65 °C with a heated lid set at 105 °C.

1. Important It is important to maintain bead suspensions at 65°C during the washing procedure below to ensure specificity of capture. Make sure that the SureSelect Wash Buffer 2 is pre-warmed to 65°C before use. Do not use a tissue incubator, or other devices with significant temperature fluctuations, for the incubation steps.
2. The hybrid capture protocol uses the SureSelect Target Enrichment Box 1 reagents (stored at room temperature), as well as Dynabeads MyOne Streptavidin T1 magnetic beads.
3. Warm the SureSelect Wash Buffer 2 at 65°C.
4. Resuspend the Dynabeads MyOne Streptavidin T1 magnetic beads by vortexing.
5. Add 50 µl of the beads to wells of a fresh PCR plate or strip tube, one well for each hybridisation sample.
6. Add 200 µl of SureSelect Binding Buffer to the beads.
7. Mix by pipetting.
8. Place on a magnetic rack, allow beads to pellet and pipette off supernatant.
9. Repeat steps 4–6 twice more for a total of three washes.
10. Resuspend the beads in 200 µl of SureSelect Binding Buffer.
11. Keep the hybridisation plate or strip tube at 65 °C. Using a multichannel pipette, transfer the whole volume (approximately 25 to 29 µl) of each hybridisation mixture from the 65 °C reaction to the plate or strip tube wells containing 200 µl of washed streptavidin beads.
12. Pipette up and down until beads are fully resuspended.
13. Seal all the wells or replace the caps on the strip tubes.
14. Incubate the plate or strip tube on a 96-well plate mixer, mixing vigorously (1400–1800 rpm) for 30 minutes at room temperature. Make sure the samples are mixing in the wells.
15. Spin down the samples in a centrifuge or mini-plate spinner.
16. Place on a magnetic rack, allow beads to pellet and pipette off supernatant.
17. Resuspend the beads in 200 µl of SureSelect Wash Buffer 1.
18. Pipette up and down until beads are fully resuspended.
19. Incubate the reaction for 15 minutes at room temperature.
20. Spin down the samples in a centrifuge or mini-plate spinner.
21. Place on a magnetic rack, allow beads to pellet and pipette off supernatant.
22. Resuspend the beads in 200 µl of Wash Buffer 2 pre-warmed at 65°C.
23. Pipette up and down until beads are fully resuspended.
24. Seal all the wells or replace the caps on the strip tubes.
25. Incubate the plate or strip tube for 10 minutes at 65 °C on the thermal cycler.
26. Place on a magnetic rack, allow beads to pellet and pipette off supernatant.
27. Repeat the wash steps 20 - 24 twice more for a total of three washes. Make sure all of the wash buffer has been removed during the final wash.
28. Add 96 µl of nuclease-free water to each sample well, and pipette up and down to resuspend the beads. Keep the samples on ice.
29. Captured DNA remains on the streptavidin beads during the post-capture amplification step.

1. Split the sample into two 48 µl aliquots.
2. Prepare the following reaction in duplicate. In 0.2 ml thin-walled PCR tubes mix the following:

   Reagent	Volume
   2x Long AMP Taq	50 µl
   PRM Adapters (10 μM)	2 µl
   Template DNA	48 µl
   Total	100 µl

3. Amplify using the following cycling conditions:

   Cycle step	Temperature	Time	No. of cycles
   Initial denaturation	95 °C	3 mins	1
   Denaturation	98 °C	20 secs	14 (b)
   Annealing	62 °C (a)	15 secs (a)	14 (b)
   Extension	65 °C (c)	3 mins	14 (b)
   Final extension	65 °C	3 mins	1
   Hold	4 °C	∞

   a. This is specific to the Oxford Nanopore primer and should be maintained

   b. Adjust accordingly if input quantities are altered

   c. This temperature is determined by the type of polymerase that is being used (given here for LongAmp Taq polymerase)

4. Place the amplified sample on a magnetic rack. Once the solution is clear, transfer the supernatant into a clean 1.5 ml Eppendorf DNA Lo-Bind tube. The beads can now be discarded.
5. Resuspend the AMPure XP beads by vortexing.
6. Add 180 µl of resuspended AMPure XP beads to the reaction and mix by pipetting.
7. Incubate on a Hula mixer (rotator mixer) for 5 minutes at room temperature.
8. Prepare sufficient fresh 70% ethanol in nuclease-free water.
9. Spin down the sample and pellet on a magnet. Keep the tube on the magnet, and pipette off the supernatant when clear and colourless.
10. Keep the tube on the magnet and wash the beads with 200 µl of freshly prepared 70% ethanol without disturbing the pellet. Remove the ethanol using a pipette and discard.
11. Repeat the previous step.
12. Spin down and place the tube back on the magnet. Pipette off any residual ethanol. Allow to dry for ~30 seconds, but do not dry the pellet to the point of cracking.
13. Remove the tube from the magnetic rack and resuspend pellet in 25 µl nuclease-free water. Incubate for 2 minutes at room temperature.
14. Pellet the beads on a magnet until the eluate is clear and colourless.
15. Remove and retain 25 µl of eluate into a clean 1.5 ml Eppendorf DNA LoBind tube. Pool the two samples together to yield 50 µl eluted sample.
16. Quantify 2 µl of amplified DNA using a Qubit fluorometer.
17. End of Step If the yield is under 500 ng, perform an additional amplification. Otherwise, proceed to Library preparation.

1. Important Perform the second round of amplification only if the DNA yield from the previous round is under 500 ng. Otherwise, proceed to Library preparation.
2. In a 0.2 ml thin-walled PCR tube mix the following:

   Reagent	Volume
   2x Long AMP Taq	50 µl
   PRM Adapters (10 μM)	2 µl
   Template DNA	48 µl
   Total	100 µl

3. Amplify using the following cycling conditions:

   Cycle step	Temperature	Time	No. of cycles
   Initial denaturation	95 °C	3 mins	1
   Denaturation	98 °C	20 secs	11 (b)
   Annealing	62 °C (a)	15 secs (a)	11 (b)
   Extension	65 °C (c)	3 mins	11 (b)
   Final extension	65 °C	3 mins	1
   Hold	4 °C	∞

   a. This is specific to the Oxford Nanopore primer and should be maintained

   b. Adjust accordingly if input quantities are altered

   c. This temperature is determined by the type of polymerase that is being used (given here for LongAmp Taq polymerase)

4. Resuspend the AMPure XP beads by vortexing.
5. Add 180 µl of resuspended AMPure XP beads to the reaction and mix by pipetting.
6. Incubate on a Hula mixer (rotator mixer) for 5 minutes at room temperature.
7. Prepare 500 μl of fresh 70% ethanol in nuclease-free water.
8. Spin down the sample and pellet on a magnet. Keep the tube on the magnet, and pipette off the supernatant when clear and colourless.
9. Keep the tube on the magnet and wash the beads with 200 µl of freshly prepared 70% ethanol without disturbing the pellet. Remove the ethanol using a pipette and discard.
10. Repeat the previous step.
11. Spin down and place the tube back on the magnet. Pipette off any residual ethanol. Allow to dry for ~30 seconds, but do not dry the pellet to the point of cracking.
12. Remove the tube from the magnetic rack and resuspend pellet in 50 µl nuclease-free water. Incubate for 2 minutes at room temperature.
13. Pellet the beads on a magnet until the eluate is clear and colourless.
14. Remove and retain 50 µl of eluate into a clean 1.5 ml Eppendorf DNA LoBind tube.
15. Quantify 2 µl of amplified DNA using a Qubit fluorometer.
16. End of Step If the yield is over 500 ng, take the amplified DNA into Library preparation.

1. Perform end repair and dA-tailing as follows:

   End-prep demo

   Mix the following reagents in a 1.5 ml Eppendorf DNA LoBind tube:

   Reagent	Volume
   ~1 µg DNA (fragmented genomic DNA, amplicon or cDNA)	45 µl
   Ultra II End-prep reaction buffer	7 µl
   Ultra II End-prep enzyme mix	3 µl
   DNA CS	5 µl
   Total	60 µl

   If using the barcoding approach the pooled input DNA should be ~1 µg in 45 µl, whether genomic, amplicon or cDNA.

2. Mix gently by flicking the tube, and spin down.
3. Transfer the sample to a 0.2 ml PCR tube, and incubate for 5 minutes at 20° C and 5 minutes at 65° C using the thermal cycler.

   If condensation is observed in the tube after the thermocycling, briefly spin down the tube contents in a microfuge.

4. Resuspend the AMPure XP beads by vortexing.
5. Transfer the sample to a clean 1.5 ml Eppendorf DNA LoBind tube.
6. Add 60 µl of resuspended AMPure XP beads to the end-prep reaction and mix by pipetting.
7. Incubate on a Hula mixer (rotator mixer) for 5 minutes at room temperature.
8. Prepare 500 μl of fresh 70% ethanol in nuclease-free water.
9. Spin down the sample and pellet on a magnet. Keep the tube on the magnet, and pipette off the supernatant when clear and colourless.
10. Keep the tube on the magnet and wash the beads with 200 µl of freshly prepared 70% ethanol without disturbing the pellet. Remove the ethanol using a pipette and discard.
11. Repeat the previous step.
12. Spin down and place the tube back on the magnet. Pipette off any residual ethanol. Allow to dry for ~30 seconds, but do not dry the pellet to the point of cracking.
13. Remove the tube from the magnetic rack and resuspend pellet in 31 µl nuclease-free water. Incubate for 2 minutes at room temperature.
14. Pellet the beads on a magnet until the eluate is clear and colourless.
15. Remove and retain 31 µl of eluate into a clean 1.5 ml Eppendorf DNA LoBind tube.
16. Quantify 1 µl of end-prepped DNA using a Qubit fluorometer - recovery aim >700 ng.

    

17. End of Step Take forward approximately 700 ng of end-prepped DNA in 30 µl nuclease-free water into adapter ligation. However, at this point, it is also possible to store the sample at 4°C overnight.

1. Important Although the recommended third-party ligase is supplied with its own buffer, the ligation efficiency of Adapter Mix (AMX) is higher when using Ligation Buffer supplied within the Ligation Sequencing Kit.
2. Spin down the Adapter Mix F (AMX-F) and Quick T4 Ligase, and place on ice.
3. Thaw Ligation Buffer (LNB) at room temperature, spin down and mix by pipetting. Due to viscosity, vortexing this buffer is ineffective. Place on ice immediately after thawing and mixing.
4. Thaw the Elution Buffer (EB) at room temperature and mix by vortexing. Then spin down and place on ice.
5. Thaw one tube of Short Fragment Buffer (SFB) at room temperature and mix by vortexing. Then spin down and place on ice.
6. In a 1.5 ml Eppendorf DNA LoBind tube, mix in the following order:

   Reagent	Volume
   DNA sample from the previous step	30 µl
   Nuclease-free water	30 µl
   Ligation Buffer (LNB)	25 µl
   NEBNext Quick T4 DNA Ligase	10 µl
   Adapter Mix F (AMX-F)	5 µl
   Total	100 µl

7. Ensure the components are thoroughly mixed by pipetting, and spin down.
8. Incubate the reaction for 10 minutes at room temperature.
9. Important If you have omitted the AMPure purification step after DNA repair and end-prep, do not incubate the reaction for longer than 10 minutes.
10. Resuspend the AMPure XP beads by vortexing.
11. Add 40 µl of resuspended AMPure XP beads to the reaction and mix by flicking the tube.
12. Incubate on a Hula mixer (rotator mixer) for 5 minutes at room temperature.
13. Spin down the sample and pellet on a magnet. Keep the tube on the magnet, and pipette off the supernatant when clear and colourless.
14. Wash the beads by adding 250 μl Short Fragment Buffer (SFB) - do NOT use Long Fragment buffer (LFB). Flick the beads to resuspend, then return the tube to the magnetic rack and allow the beads to pellet. Remove the supernatant using a pipette and discard.
15. Repeat the previous step.
16. Spin down and place the tube back on the magnet. Pipette off any residual supernatant. Allow to dry for ~30 seconds, but do not dry the pellet to the point of cracking.
17. Remove the tube from the magnetic rack and resuspend the pellet in 15 µl Elution Buffer (EB). Spin down and incubate for 10 minutes at room temperature. For high molecular weight DNA, incubating at 37°C can improve the recovery of long fragments.
18. Pellet the beads on a magnet until the eluate is clear and colourless, for at least 1 minute.
19. Remove and retain 15 µl of eluate containing the DNA library into a clean 1.5 ml Eppendorf DNA LoBind tube.

    Dispose of the pelleted beads

20. End of Step The prepared library is used for loading into the flow cell. Store the library on ice or at 4°C until ready to load.
21. Tip Library storage recommendations

    We recommend storing libraries in Eppendorf DNA LoBind tubes at 4°C for short term storage or repeated use, for example, reloading flow cells between washes.
    For single use and long-term storage of more than 3 months, we recommend storing libraries at -80°C in Eppendorf DNA LoBind tubes.
    For further information, please refer to the DNA library stability Know-How document.

22. Optional Action

    If quantities allow, the library may be diluted in Elution Buffer (EB) for splitting across multiple flow cells.

    Additional buffer for doing this can be found in the Sequencing Auxiliary Vials expansion (EXP-AUX002), available to purchase separately. This expansion also contains additional vials of Sequencing Buffer II (SQII) and Loading Beads II (LBII), required for loading the libraries onto flow cells.

1. Tip Priming and loading a MinION flow cell

   We recommend all new users watch the 'Priming and loading your flow cell' video before your first run.

2. Using the Loading Solution

   We recommend using the Loading Beads II (LBII) for loading your library onto the flow cell for most sequencing experiments. However, if you have previously used water to load your library, you must use Loading Solution (LS) instead of water.
   Note: some customers have noticed that viscous libraries can be loaded more easily when not using Loading Beads II.

3. Thaw the Sequencing Buffer II (SBII), Loading Beads II (LBII) or Loading Solution (LS, if using), Flush Tether (FLT) and one tube of Flush Buffer (FB) at room temperature before mixing the reagents by vortexing and spin down at room temperature.
4. To prepare the flow cell priming mix, add 30 µl of thawed and mixed Flush Tether (FLT) directly to the tube of thawed and mixed Flush Buffer (FB), and mix by vortexing at room temperature.
5. Open the MinION device lid and slide the flow cell under the clip.

   Press down firmly on the flow cell to ensure correct thermal and electrical contact.

   

   

6. Optional Action

   Complete a flow cell check to assess the number of pores available before loading the library.

   This step can be omitted if the flow cell has been checked previously.

   See the flow cell check instructions in the MinKNOW protocol for more information.

7. Slide the flow cell priming port cover clockwise to open the priming port.

   

8. Important Take care when drawing back buffer from the flow cell. Do not remove more than 20-30 µl, and make sure that the array of pores are covered by buffer at all times. Introducing air bubbles into the array can irreversibly damage pores.
9. After opening the priming port, check for a small air bubble under the cover. Draw back a small volume to remove any bubbles:
   1. Set a P1000 pipette to 200 µl
   2. Insert the tip into the priming port
   3. Turn the wheel until the dial shows 220-230 µl, to draw back 20-30 µl, or until you can see a small volume of buffer entering the pipette tip
      

   Note: Visually check that there is continuous buffer from the priming port across the sensor array.

   

10. Load 800 µl of the priming mix into the flow cell via the priming port, avoiding the introduction of air bubbles. Wait for five minutes. During this time, prepare the library for loading by following the steps below.

    

11. Thoroughly mix the contents of the Loading Beads II (LBII) by pipetting.
12. Important The Loading Beads II (LBII) tube contains a suspension of beads. These beads settle very quickly. It is vital that they are mixed immediately before use.
13. In a new tube, prepare the library for loading as follows:

    Reagent	Volume per flow cell
    Sequencing Buffer II (SBII)	37.5 µl
    Loading Beads II (LBII) mixed immediately before use, or Loading Solution (LS), if using	25.5 µl
    DNA library	12 µl
    Total	75 µl

    Note: Load the library onto the flow cell immediately after adding the Sequencing Buffer II (SBII) and Loading Beads II (LBII).

14. Complete the flow cell priming:
    1. Gently lift the SpotON sample port cover to make the SpotON sample port accessible.
    2. Load 200 µl of the priming mix into the flow cell priming port (not the SpotON sample port), avoiding the introduction of air bubbles.

    

    

15. Mix the prepared library gently by pipetting up and down just prior to loading.
16. Add 75 μl of the prepared library to the flow cell via the SpotON sample port in a dropwise fashion. Ensure each drop flows into the port before adding the next.

    

17. Gently replace the SpotON sample port cover, making sure the bung enters the SpotON port, close the priming port and replace the MinION device lid.

    

    

1. How to start sequencing

   Once you have loaded your flow cell, the sequencing run can be started on MinKNOW, our sequencing software that controls the device, data acquisition and real-time basecalling. For more detailed information on setting up and using MinKNOW, please see the MinKNOW protocol.

   MinKNOW can be used and set up to sequence in multiple ways:

   • On a computer either directly or remotely connected to a sequencing device.
   • Directly on a GridION, MinION Mk1C or PromethION 24/48 sequencing device.

   For more information on using MinKNOW on a sequencing device, please see the device user manuals:

   • MinION Mk1B user manual
   • MinION Mk1C user manual
   • GridION user manual

   ---

   To start a sequencing run on MinKNOW:

   1. Navigate to the start page and click Start sequencing.

   2. Fill in your experiment details, such as name and flow cell position and sample ID.

   3. Select the sequencing kit used in the library preparation on the Kit page.

   4. Configure the sequencing and output parameters for your sequencing run or keep to the default settings on the Run configuration tab.

   Note: If basecalling was turned off when a sequencing run was set up, basecalling can be performed post-run on MinKNOW. For more information, please see the MinKNOW protocol.

   5. Click Start to initiate the sequencing run.

2. Data analysis after sequencing

   After sequencing has completed on MinKNOW, the flow cell can be reused or returned, as outlined in the Flow cell reuse and returns section.

   After sequencing and basecalling, the data can be analysed. For further information about options for basecalling and post-basecalling analysis, please refer to the Data Analysis document.

   In the Downstream analysis section, we outline further options for analysing your data.

1. After your sequencing experiment is complete, if you would like to reuse the flow cell, please follow the Flow Cell Wash Kit protocol and store the washed flow cell at 2-8°C.

   The Flow Cell Wash Kit protocol is available on the Nanopore Community.

2. Tip We recommend you to wash the flow cell as soon as possible after you stop the run. However, if this is not possible, leave the flow cell on the device and wash it the next day.
3. Alternatively, follow the returns procedure to flush out the flow cell ready to send back to Oxford Nanopore.

   Instructions for returning flow cells can be found here.

   Note: All flow cells must be flushed with deionised water before returning the product.

4. Important If you encounter issues or have questions about your sequencing experiment, please refer to the Troubleshooting Guide that can be found in the online version of this protocol.

1. Post-basecalling analysis

   There are several options for further analysing your basecalled data:

   1. EPI2ME workflows

   For in-depth data analysis, Oxford Nanopore Technologies offers a range of bioinformatics tutorials and workflows available in EPI2ME. The platform provides a vehicle where workflows deposited in GitHub by our Research and Applications teams can be showcased with descriptive texts, functional bioinformatics code and example data.

   2. Research analysis tools

   Oxford Nanopore Technologies' Research division has created a number of analysis tools, which are available in the Oxford Nanopore GitHub repository. The tools are aimed at advanced users, and contain instructions for how to install and run the software. They are provided as-is, with minimal support.

   3. Community-developed analysis tools

   If a data analysis method for your research question is not provided in any of the resources above, please refer to the resource centre and search for bioinformatics tools for your application. Numerous members of the Nanopore Community have developed their own tools and pipelines for analysing nanopore sequencing data, most of which are available on GitHub. Please be aware that these tools are not supported by Oxford Nanopore Technologies, and are not guaranteed to be compatible with the latest chemistry/software configuration.

1. Below is a list of the most commonly encountered issues, with some suggested causes and solutions.

   We also have an FAQ section available on the Nanopore Community Support section.

   If you have tried our suggested solutions and the issue still persists, please contact Technical Support via email (support@nanoporetech.com) or via LiveChat in the Nanopore Community.

2. Low sample quality

   Observation	Possible cause	Comments and actions
   Low DNA purity (Nanodrop reading for DNA OD 260/280 is <1.8 and OD 260/230 is <2.0–2.2)	The DNA extraction method does not provide the required purity	The effects of contaminants are shown in the Contaminants document. Please try an alternative extraction method that does not result in contaminant carryover. Consider performing an additional SPRI clean-up step.
   Low RNA integrity (RNA integrity number <9.5 RIN, or the rRNA band is shown as a smear on the gel)	The RNA degraded during extraction	Try a different RNA extraction method. For more info on RIN, please see the RNA Integrity Number document. Further information can be found in the DNA/RNA Handling page.
   RNA has a shorter than expected fragment length	The RNA degraded during extraction	Try a different RNA extraction method. For more info on RIN, please see the RNA Integrity Number document. Further information can be found in the DNA/RNA Handling page. We recommend working in an RNase-free environment, and to keep your lab equipment RNase-free when working with RNA.

3. Low DNA recovery after AMPure bead clean-up

   Observation	Possible cause	Comments and actions
   Low recovery	DNA loss due to a lower than intended AMPure beads-to-sample ratio	1. AMPure beads settle quickly, so ensure they are well resuspended before adding them to the sample. 2. When the AMPure beads-to-sample ratio is lower than 0.4:1, DNA fragments of any size will be lost during the clean-up.
   Low recovery	DNA fragments are shorter than expected	The lower the AMPure beads-to-sample ratio, the more stringent the selection against short fragments. Please always determine the input DNA length on an agarose gel (or other gel electrophoresis methods) and then calculate the appropriate amount of AMPure beads to use.
   Low recovery after end-prep	The wash step used ethanol <70%	DNA will be eluted from the beads when using ethanol <70%. Make sure to use the correct percentage.

1. Below is a list of the most commonly encountered issues, with some suggested causes and solutions.

   We also have an FAQ section available on the Nanopore Community Support section.

   If you have tried our suggested solutions and the issue still persists, please contact Technical Support via email (support@nanoporetech.com) or via LiveChat in the Nanopore Community.

2. Fewer pores at the start of sequencing than after Flow Cell Check

   Observation	Possible cause	Comments and actions
   MinKNOW reported a lower number of pores at the start of sequencing than the number reported by the Flow Cell Check	An air bubble was introduced into the nanopore array	After the Flow Cell Check it is essential to remove any air bubbles near the priming port before priming the flow cell. If not removed, the air bubble can travel to the nanopore array and irreversibly damage the nanopores that have been exposed to air. The best practice to prevent this from happening is demonstrated in this video.
   MinKNOW reported a lower number of pores at the start of sequencing than the number reported by the Flow Cell Check	The flow cell is not correctly inserted into the device	Stop the sequencing run, remove the flow cell from the sequencing device and insert it again, checking that the flow cell is firmly seated in the device and that it has reached the target temperature. If applicable, try a different position on the device (GridION/PromethION).
   MinKNOW reported a lower number of pores at the start of sequencing than the number reported by the Flow Cell Check	Contaminations in the library damaged or blocked the pores	The pore count during the Flow Cell Check is performed using the QC DNA molecules present in the flow cell storage buffer. At the start of sequencing, the library itself is used to estimate the number of active pores. Because of this, variability of about 10% in the number of pores is expected. A significantly lower pore count reported at the start of sequencing can be due to contaminants in the library that have damaged the membranes or blocked the pores. Alternative DNA/RNA extraction or purification methods may be needed to improve the purity of the input material. The effects of contaminants are shown in the Contaminants Know-how piece. Please try an alternative extraction method that does not result in contaminant carryover.

3. MinKNOW script failed

   Observation	Possible cause	Comments and actions
   MinKNOW shows "Script failed"		Restart the computer and then restart MinKNOW. If the issue persists, please collect the MinKNOW log files and contact Technical Support. If you do not have another sequencing device available, we recommend storing the flow cell and the loaded library at 4°C and contact Technical Support for further storage guidance.

4. Pore occupancy below 40%

   Observation	Possible cause	Comments and actions
   Pore occupancy <40%	Not enough library was loaded on the flow cell	Ensure you load the recommended amount of good quality library in the relevant library prep protocol onto your flow cell. Please quantify the library before loading and calculate mols using tools like the Promega Biomath Calculator, choosing "dsDNA: µg to pmol"
   Pore occupancy close to 0	The Ligation Sequencing Kit was used, and sequencing adapters did not ligate to the DNA	Make sure to use the NEBNext Quick Ligation Module (E6056) and Oxford Nanopore Technologies Ligation Buffer (LNB, provided in the sequencing kit) at the sequencing adapter ligation step, and use the correct amount of each reagent. A Lambda control library can be prepared to test the integrity of the third-party reagents.
   Pore occupancy close to 0	The Ligation Sequencing Kit was used, and ethanol was used instead of LFB or SFB at the wash step after sequencing adapter ligation	Ethanol can denature the motor protein on the sequencing adapters. Make sure the LFB or SFB buffer was used after ligation of sequencing adapters.
   Pore occupancy close to 0	No tether on the flow cell	Tethers are adding during flow cell priming (FLT/FCT tube). Make sure FLT/FCT was added to FB/FCF before priming.

5. Shorter than expected read length

   Observation	Possible cause	Comments and actions
   Shorter than expected read length	Unwanted fragmentation of DNA sample	Read length reflects input DNA fragment length. Input DNA can be fragmented during extraction and library prep. 1. Please review the Extraction Methods in the Nanopore Community for best practice for extraction. 2. Visualise the input DNA fragment length distribution on an agarose gel before proceeding to the library prep. In the image above, Sample 1 is of high molecular weight, whereas Sample 2 has been fragmented. 3. During library prep, avoid pipetting and vortexing when mixing reagents. Flicking or inverting the tube is sufficient.

6. Large proportion of unavailable pores

   Observation	Possible cause	Comments and actions
   Large proportion of unavailable pores (shown as blue in the channels panel and pore activity plot) The pore activity plot above shows an increasing proportion of "unavailable" pores over time.	Contaminants are present in the sample	Some contaminants can be cleared from the pores by the unblocking function built into MinKNOW. If this is successful, the pore status will change to "sequencing pore". If the portion of unavailable pores stays large or increases: 1. A nuclease flush using the Flow Cell Wash Kit (EXP-WSH004) can be performed, or 2. Run several cycles of PCR to try and dilute any contaminants that may be causing problems.

7. Large proportion of inactive pores

   Observation	Possible cause	Comments and actions
   Large proportion of inactive/unavailable pores (shown as light blue in the channels panel and pore activity plot. Pores or membranes are irreversibly damaged)	Air bubbles have been introduced into the flow cell	Air bubbles introduced through flow cell priming and library loading can irreversibly damage the pores. Watch the Priming and loading your flow cell video for best practice
   Large proportion of inactive/unavailable pores	Certain compounds co-purified with DNA	Known compounds, include polysaccharides, typically associate with plant genomic DNA. 1. Please refer to the Plant leaf DNA extraction method. 2. Clean-up using the QIAGEN PowerClean Pro kit. 3. Perform a whole genome amplification with the original gDNA sample using the QIAGEN REPLI-g kit.
   Large proportion of inactive/unavailable pores	Contaminants are present in the sample	The effects of contaminants are shown in the Contaminants Know-how piece. Please try an alternative extraction method that does not result in contaminant carryover.

8. Reduction in sequencing speed and q-score later into the run

   Observation	Possible cause	Comments and actions
   Reduction in sequencing speed and q-score later into the run	For Kit 9 chemistry (e.g. SQK-LSK109), fast fuel consumption is typically seen when the flow cell is overloaded with library (please see the appropriate protocol for your DNA library to see the recommendation).	Add more fuel to the flow cell by following the instructions in the MinKNOW protocol. In future experiments, load lower amounts of library to the flow cell.

9. Temperature fluctuation

   Observation	Possible cause	Comments and actions
   Temperature fluctuation	The flow cell has lost contact with the device	Check that there is a heat pad covering the metal plate on the back of the flow cell. Re-insert the flow cell and press it down to make sure the connector pins are firmly in contact with the device. If the problem persists, please contact Technical Services.

10. Failed to reach target temperature

    Observation	Possible cause	Comments and actions
    MinKNOW shows "Failed to reach target temperature"	The instrument was placed in a location that is colder than normal room temperature, or a location with poor ventilation (which leads to the flow cells overheating)	MinKNOW has a default timeframe for the flow cell to reach the target temperature. Once the timeframe is exceeded, an error message will appear and the sequencing experiment will continue. However, sequencing at an incorrect temperature may lead to a decrease in throughput and lower q-scores. Please adjust the location of the sequencing device to ensure that it is placed at room temperature with good ventilation, then re-start the process in MinKNOW. Please refer to this FAQ for more information on MinION temperature control.

11. Guppy – no input .fast5 was found or basecalled

    Observation	Possible cause	Comments and actions
    No input .fast5 was found or basecalled	input_path did not point to the .fast5 file location	The --input_path has to be followed by the full file path to the .fast5 files to be basecalled, and the location has to be accessible either locally or remotely through SSH.
    No input .fast5 was found or basecalled	The .fast5 files were in a subfolder at the input_path location	To allow Guppy to look into subfolders, add the --recursive flag to the command

12. Guppy – no Pass or Fail folders were generated after basecalling

    Observation	Possible cause	Comments and actions
    No Pass or Fail folders were generated after basecalling	The --qscore_filtering flag was not included in the command	The --qscore_filtering flag enables filtering of reads into Pass and Fail folders inside the output folder, based on their strand q-score. When performing live basecalling in MinKNOW, a q-score of 7 (corresponding to a basecall accuracy of ~80%) is used to separate reads into Pass and Fail folders.

13. Guppy – unusually slow processing on a GPU computer

    Observation	Possible cause	Comments and actions
    Unusually slow processing on a GPU computer	The --device flag wasn't included in the command	The --device flag specifies a GPU device to use for accelerate basecalling. If not included in the command, GPU will not be used. GPUs are counted from zero. An example is --device cuda:0 cuda:1, when 2 GPUs are specified to use by the Guppy command.