Dec 12, 2025
Nanopore Sequencing of poliovirus isolates
- Catherine Troman1,
- Erika Bujaki2,
- Ben Bellekom1,
- Joyce Akello1,
- Shannon Fitz1,
- Alex Shaw1,
- Javier Martin1,
- Nick Grassly1
- 1Imperial College London;
- 2MHRA
- Poliovirus Sequencing Consortium
Protocol Citation: Catherine Troman, Erika Bujaki, Ben Bellekom, Joyce Akello, Shannon Fitz, Alex Shaw, Javier Martin, Nick Grassly 2025. Nanopore Sequencing of poliovirus isolates. protocols.io https://dx.doi.org/10.17504/protocols.io.q26g7nq79lwz/v1
License: This is an open access protocol distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited
Protocol status: Working
We use this protocol and it's working
Created: December 12, 2025
Last Modified: December 12, 2025
Protocol Integer ID: 234855
Keywords: polio, poliovirus, nanopore, DDNS, isolates, direct detection, nanopore sequencing of poliovirus, nanopore sequencing, vp1 region of poliovirus, direct detection of poliovirus, use with oxford nanopore v14 chemistry, sequencing reagent, poliovirus, oxford nanopore v14 chemistry, gridion sequencer, primer sequence, single pcr, y7 primer set, minion mk1b, y7 primer, cell culture isolate, primer, sequencing
Funders Acknowledgements:
Bill and Melinda Gates Foundations
Grant ID: INV-052182
Abstract
This protocol is adapted from "Direct Detection of poliovirus and Nanopore Sequencing (DDNS) - Stool" to make it suitable for use with cell culture isolates in either a liquid form or that have been transported to the lab via FTA card.
The protocol aims to amplify the VP1 region of poliovirus through a single PCR using the Q8/Y7 primer set. We use barcoded primers as this greatly simplifies the subsequent library preparation process. Primer sequences for the barcoded Q8/Y7 primers are found in Dataset S1 of Shaw et al (2020).
This protocol is for use with Oxford Nanopore v14 chemistry sequencing reagents and can be used with the MinION Mk1B or GridION sequencer.
Within the protocol, quality control steps are included which when followed ensures the validity of your results and provides easier troubleshooting when needed.
Materials
Nanopore Flow Cell R10.4.1Oxford Nanopore TechnologiesCatalog #FLO-MIN114
Nuclease-free Water
0.2mL PCR tubes
1.5mL DNA LoBind tubesEppendorfCatalog #0030108051
100% Molecular Biology Grade Ethanol
Protocol materials
SuperScript III One-Step RT-PCR System with Platinum TaqInvitrogen - Thermo FisherCatalog #12457-026
Agencourt AMPure XPBeckman CoulterCatalog #A63880
ONT Flow Cell Wash KitOxford Nanopore TechnologiesCatalog #EXP-WSH004
NEBNext Ultra End Repair/dA-Tailing Module - 96 rxnsNew England BiolabsCatalog #E7442L
NEBNext Quick Ligation Module - 20 rxnsNew England BiolabsCatalog #E6056S
Ligation Sequencing Kit V14Oxford Nanopore TechnologiesCatalog #SQK-LSK114
Ultrapure BSAAmbionCatalog #AM2616
Troubleshooting
Before start
This protocol describes the amplification of the VP1 region and library preparation for sequencing poliovirus isolates. We anticipate users will have performed an RNA extraction prior to starting this protocol. We recommend the MagMAX Viral RNA Isolation Kit for this process.
Barcoded VP1 Primers:
To allow a simplified protocol, we use a 96-well primer plate with 5µM barcoded Y7 primer and 5µM barcoded Q8 primer in each well.
Each well contains Q8 and Y7 primers with the same unique barcode e.g A1 = Y7 with barcode 1 and Q8 with barcode 1, A2 = Y7 with barcode 2 and Q8 with barcode 2, etc. The full set of 96 barcoded primer sequences are shown in Dataset_S1 of Shaw et al, 2020.
These primers can be ordered premixed or as two separate plates then mixed in the lab.
Sample Organisation
30m
Only isolates providing ITD results that would normally be put forward for sequencing should be sequenced using this protocol.
This would be isolates that provide one of the following results after performing ITD:
- PV1
- SL1 discordant
- SL3 discordant
- Any Type 2 poliovirus
Pairs of samples (with the same EPID) can have consecutive barcodes but try not to group samples from the same geographic area together. This helps detect any potential cross-contamination because identical sequences are then unlikely to be detected in samples with consecutive barcodes that are adjacent to one another on the 96-well plate.
Record sample data, and the order for the samples in your csv file. At this point you can also add any other metadata that you have for the samples.
Here is an example of a sample csv file: 
isolate_template_v4.csv0B
isolate_template_v4.csv0B It is advised that you edit the name of the file so it is unique for each run you analyse.
You should also include any positive and negative controls in your list of samples. A positive control (resuspended Coxsackievirus A20 provided by MHRA) and negative control (nuclease free water) should each be included on the first and last RNA extraction batches of the day at least.
If any samples are repeats from a previous run, note this down in the appropriate column.
If there has been a delay in the processing of the sample e.g. due to a lack of extraction kits or software updates preventing the run, note "Yes" in the column "DelaysInProcessingForSequencing" and enter the type of delay in the column "DetailsOfDelays".
Note
Do not include any personal information from the patients in your csv file, and avoid using special characters in any of the metadata columns, including the sample names (stick to - or _).
30m
For batching samples into a run, we recommend performing a sequencing run at least once every two weeks with up to 48 samples (including any positive and negative controls).
This frequency avoids causing too long a delay between sequencing runs when waiting for sample numbers to build up for batching together.
rt-PCR (barcoded VP1)
6h 30m
Wipe down lab bench surfaces and pipettes with 70% Ethanol and an RNAse specific decontaminant, such as RNAse Zap.
Prepare a master mix using the reaction volumes detailed in the table below for the number of samples you have plus negative controls. The reaction mix and SSIII enzyme are provided in SuperScript III One-Step RT-PCR System with Platinum TaqInvitrogen - Thermo FisherCatalog #12457-026
| A | B | |
| Reagent | 1 reaction (μL) | |
| 2x Reaction mix | 12.5 | |
| Nuclease Free Water | 4.5 | |
| SSIII Platinum Taq mix | 1 |
30m
Vortex the mastermix for 3 seconds and spin down for 5 seconds to gather contents at the bottom of the tube. Aliquot 18μL to each 0.2mL PCR tube.
Add 2μL of barcoded primer to each well, ensuring you add a different barcode for each reaction.
Add 5μL sample RNA to each reaction, and 5μL of nuclease free water for negative controls, and pipette 5 times to mix
20m
Spin down for 5 seconds to make sure all reagents are in the bottom of the tube.
10s
Amplify using the following cycling conditions:
| A | B | C | D | |
| Cycle | Step | Temperature (°C) | Time | |
| 1 | Reverse transcription | 50 | 30 minutes | |
| 1 | Initial denaturing | 94 | 2 minutes | |
| 42 | Denaturing | 94 | 15 seconds | |
| Annealing | 55 | 30 seconds | ||
| Extension | 68 | 2 minutes | ||
| 1 | Final extension | 68 | 5 minutes | |
| - | Hold | 10 | - |
3h
Once the PCR is finished, check to see if any reactions have evaporated, if so, note this down in the sample csv.
5m
Check all positive and negative controls on a 1% agarose gel. The expected band for the positive control is around 1.2kb.
All samples can be marked as “Pass” for the PositiveControlCheck if all positive controls extracted on the same day show a VP1 band on the gel.
All samples can be marked as “Pass” for the NegativeControlCheck if all negative controls extracted on the same day show no VP1 band on the gel.
If any positive controls fail, or any negative controls have a band, all samples must be marked as fail.
1h
If there is no band for the positive control, repeat the rtPCR for the controls only.
If a band is visible after repeating, discard the previous VP1 amplicons and repeat the VP1 reactions for all samples.
If there is no band visible after repeating the PCR, repeat the RNA extractions after checking the RNA extraction kit is being used correctly and has not expired.
1h
If the negative control check is failed, repeat the rtPCR.
If the negative control still shows a band on a gel or tapestation:
- Thoroughly clean the PCR and RNA extraction workstations.
- Replace each of the PCR reagents in turn whilst performing blank reactions to determine a contaminated reagent.
- Perform an additional Negative RNA extraction to confirm that that RNA extraction kit is not contaminated.
30m
Library Preparation for ONT MinION: Pooling, End-Prep and Adapter Ligation
1h 45m
Wipe down lab bench surfaces and pipettes with 70% Ethanol and a DNA specific decontaminant, such as DNA Away.
Pool 2μL of each VP1 product into a clean 1.5mL tube and concentrate with AMPure beads
Agencourt AMPure XPBeckman CoulterCatalog #A63880
5m
Add a volume of AMPure beads equal to the volume of the pooled VP1 products and incubate at room temperature for 5 minutes. Flick gently after 2 minutes to aid binding.
e.g. 40 samples, 2μL each pooled = 80μL pool, so add 80μL AMPure beads
6m
Spin down the tube for 3 seconds then place on a magnetic rack until all the beads have formed a pellet and the solution is clear.
3m
Pipette off the solution, avoiding disturbing the bead pellet.
1m
Add 200μL of 80% Ethanol to the tube, leave for 30 seconds, then remove and discard.
Repeat this step.
2m
Spin down the tube for 2 seconds, place back on the magnet, then remove any remaining Ethanol.
Allow the pellet to air dry for 30 seconds or until dry but not cracking
1m
Take the tube off the magnet and add 51μL of nuclease free water. Flick the tube to resuspend the beads and incubate at room temperature for 2 minutes.
3m
Spin down the tube for 3 seconds then place back on the magnet, allowing the beads to pellet completely.
30s
Remove 50μL of the eluted DNA and add to a clean 0.2mL PCR tube.
30s
End-preparation:
Add the following reagents from NEBNext Ultra End Repair/dA-Tailing Module - 96 rxnsNew England BiolabsCatalog #E7442L to the 0.2mL tube containing the cleaned DNA pool.
| A | B | |
| Reagent | Volume (μL) | |
| UltraII End-Prep reaction buffer | 7 | |
| UltraII End-prep enzyme mix | 3 |
2m
Mix gently by flicking the tube and spin down for 3 seconds.
1m
In the thermocycler, incubate for 5 minutes at 20°C followed by 5 minutes at 65°C
10m
Transfer to a 1.5mL tube and perform an AMPure bead clean.
15m
Vortex the AMPure beads until all the beads are well mixed.
30s
Add 60μl of resuspended beads to the tube and flick the tube to mix.
Incubate at room temperature for 5 minutes. Flick gently after 2 minutes to aid binding.
5m
Spin down the tube for 3 seconds then place on a magnetic rack until all the beads have formed a pellet and the solution is clear.
1m
Pipette off the solution, avoiding disturbing the bead pellet.
1m
Add 200μL of 80% Ethanol to the tube, leave for 30seconds, then remove and discard.
Repeat.
2m
Spin down the tube for 2 seconds, place back on the magnet, then remove any remaining Ethanol.
Allow the pellet to air dry for 1 minute or until dry but not cracking
2m
Take the tube off the magnet and add 61μL of nuclease free water. Flick the tube to resuspend the beads and incubate at room temperature for 2 minutes.
3m
Spin down the tube for 3 seconds then place back on the magnet, allowing the beads to pellet completely.
1m
Remove 60μL of the eluted DNA and add to a clean 1.5mL tube.
Note
At this point you can store the end-prepared library at 4°C. This can be stored for up to one week before continuing to step 14, however it is advised to continue the library preparation protocol as soon as possible.
Ensure you label the tube clearly with the run name and what stage of the library preparation you were at e.g. 20240229 DDNSrun10 end-prep
30s
From NEBNext Quick Ligation Module - 20 rxnsNew England BiolabsCatalog #E6056S
Spin down the NEB Quick T4 Ligase and place on ice.
From Ligation Sequencing Kit V14Oxford Nanopore TechnologiesCatalog #SQK-LSK114
Spin down and thaw Ligation Adapter (LA) on ice.
Thaw Ligation Buffer (LNB) at room temperature, spin down, mix by pipetting, then place on ice.
Thaw Elution Buffer (EB), and Short Fragment Buffer (SFB) at room temperature, mix by vortexing then place on ice.
If you plan to start the run on the same day, remove the Flush buffer, flush tether (FLT) and Ultrapure BSAAmbionCatalog #AM2616 from the freezer and thaw at room temperature. Once thawed, place on ice.
Remove your flow cell from the fridge to allow it to get to room temperature.
3m
Prepare the following reaction mix adding reagents to the 1.5mL tube with 60μL end-prepped DNA:
| A | B | |
| Reagent | Volume (μL) | |
| Ligation buffer (LNB) | 25 | |
| Ligation adapter (LA) | 5 | |
| NEB Quick T4 Ligase | 10 |
2m
Mix gently by flicking the tube then spin down for 3 seconds
1m
Incubate at room temperature for 10 minutes
10m
During this time, you can run your flow cell check
Plug in your sequencing device, open the lid and insert your flowcell. In the MinKNOW software, navigate to the start panel then select flowcell check, then start. This will tell you how many pores are available for sequencing.
If your flow cell has been used before, instead of running a flow cell check, start a dummy sequencing run by selecting Start Sequencing, name the run "flowcell_check", select any kit, then set the time to 10 minutes, skip to final review then start run. At the beginning of the run it will do a short flow cell check and give a more accurate number for the available pores (calculated by adding together the available and unavailable pores in the pore status graph (see example image below)).
If a flow cell has less than 700 pores, do not use it for a 48 sample DDNS isolate run. Take out a different flow cell and perform a flow cell check. The number of pores available in the flow cell you use should be noted down in the sample csv in the column “PoresAvilableAtFlowCellCheck” and the flow cell ID should be recorded in the “FlowCellID” column. Also record the number of times the flow cell has been used in the column “FlowCellUses”.
Carry out an AMPure bead purification using 40μL of resuspended AMPure XP beads.
Note: This clean-up is different to previous as it uses the ONT Short Fragment Buffer (SFB) and Elution buffer (EB) instead of 80% ethanol and water.
Vortex the AMPure beads until all the beads are well mixed.
30s
Add 40μL of resuspended beads to the 1.5mL tube and mix by flicking the tube.
Incubate at room temperature for 5 minutes. Flick gently after 2 minutes to aid binding.
6m
Spin down the tube for 3 seconds then place on a magnetic rack until all the beads have formed a pellet and the solution is clear.
1m
Pipette off the solution, avoiding disturbing the bead pellet.
30s
Add 250μL of Short Fragment Buffer (SFB). Remove the tube from the magnet and resuspend the beads in the SFB by flicking the tube.
Spin down for 3 seconds then return the tube to the magnet.
Allow the beads to pellet, then remove and discard.
Repeat.
4m
Spin down the tube for 2 seconds, place back on the magnet, then remove any remaining SFB.
Allow the pellet to air dry for 1 minute or until dry but not cracked
1m
Take the tube off the magnet and add 15μL of Elution buffer (EB). Flick gently to resuspend the beads and incubate at room temperature for 10 minutes.
10m
Spin down the tube for 3 seconds then place back on the magnet, allowing the beads to pellet completely.
1m
Remove 12μL of the eluted DNA and transfer to a clean 1.5mL tube.
Note
At this point you can keep your prepared library at 4°C overnight with minimal loss of throughput. This can be kept for up to two weeks before sequencing, however we recommend that you continue to flow cell loading as soon as possible.
Ensure you label the tube clearly with the run name and what stage of the library preparation you were at e.g. 20240229 DDNSrun10 final library.
30s
Priming and Loading the flowcell
30m
Thaw the Sequencing buffer (SB), Library beads (LIB), Flow Cell Tether (FCT) and one tube of Flow Cell Flush (FCF) at room temperature then place on ice.
Mix the SQB, FCF, and FCT by vortexing, spin down, and return to ice. Spin down the LIB then place back on ice.
10m
To create the priming mix, combine the following reagents in a clean 1.5mL tube:
| A | B | |
| Reagent | Volume (μL) | |
| Flow cell flush (FCF) | 1,170 | |
| Flow cell tether (FCT) | 30 | |
| BSA (50mg/mL) | 5 |
Mix by pipetting and spin down. Place on ice until ready to use.
2m
Open the lid of the nanopore sequencing device and slide the flow cell's priming port cover clockwise so that the priming port is visible. After opening the priming port, check for any bubbles under the cover. Draw back a small volume to remove any bubbles (a few µLs). Visually check that there is continuous buffer from the priming port across the sensor array.
3m
Using a P1000 pipette, slowly load 800μL of the priming mix into the flow cell via the priming port.
Leave a small amount of liquid in the end of the pipette tip to ensure you do not introduce air into the flowcell.
Leave for 5 minutes.
2m
Mix the contents of the LIB tube by pipetting just before adding to the following library mix in the 1.5ml tube with your DNA library:
| A | B | |
| Reagent | Volume (μL) | |
| Sequencing buffer (SB) | 37.5 | |
| Library beads (LIB) | 25.5 |
2m
Complete the flowcell priming by opening the SpotOn port cover and carefully loading 200μL of the priming mix into the priming port. As before, leave a small amount of liquid in the bottom of the tip to avoid the introduction of air bubbles.
When adding the priming mix, you may see a small amount of liquid come up through the SpotOn port. If you do, pause and allow the liquid to flow back into the flowcell before continuing putting through the priming mix.
2m
Mix the prepared library mix gently by pipetting.
Add the library mix to the flowcell via the SpotOn port in a dropwise fashion, allowing each drop to flow into the flowcell before adding the next.
2m
Replace the SpotOn port cover and close the priming port, then replace the lid of your sequencing device.
1m
Starting the sequencing run
5m 30s
Open the ONT MinKNOW software and follow the steps below to set up and start your sequencing run.
30s
Click start, then start sequencing.
Create a name for you sequencing run, it is good practise to make this unique and identifiable for if you ever need to revisit the data. The date and an experiment name are recommended. In sample name you can put a number or repeat the experiment name - this is not as important as the run name. Then click continue.
1m
Select the kit used - this is SQK-LSK114. Once you click this the barcoding options will appear. Select EXP-PBC096, then click continue
30s
In the run length options, set the run time to 7 hours for a run of 40 samples (approximately 10 minutes per sample rounded up to the nearest hour). Click continue.
30s
In the basecalling options, select high accuracy basecalling. In the barcoding options, make sure barcoding is enabled and toggle to use barcode at both ends. Click continue until you reach the run overview, where you can double check the selected options, then click start run.
1m
In your sample csv, record the run number in the column "RunNumber", the date in "DateSeqRunLoaded", and the run duration in "RunHoursDuration".
2m
Washing the flow cell
1h 30m
After the sequencing run is finished you can wash your flow cell to remove the remaining library and either prepare for another sequencing run or for storage at 4°C. The wash uses the reagents supplied in the ONT wash kit:
ONT Flow Cell Wash KitOxford Nanopore TechnologiesCatalog #EXP-WSH004
Thaw the Wash Diluent at room temperature and mix briefly by vortexing.
Spin down the tube of wash mix (WMX) and place on ice.
10m
Prepare the following wash solution in a clean 1.5mL tube
| A | B | |
| Reagent | Volume (μL) | |
| Wash diluent | 398 | |
| Wash mix (WMX) | 2 |
5m
Open the Priming port and using a P1000 pipette, carefully remove a small amount of liquid to remove any air bubbles under the port.
2m
Carefully add 200μL of the wash solution through the priming port, leaving a small amount of liquid in the tip towards the end to avoid introducing an air bubble.
Close the priming port and incubate at room temperature for 5 minutes.
5m
Carefully add the remaining 200μL of wash solution through the priming port, again leaving a small amount of liquid in the tip towards the end to avoid introducing an air bubble.
Close the priming port and incubate at room temperature for 1 hour.
1h 1m
At this point you can remove all waste from the waste channel, ensuring that the Priming Port is closed before doing so.
You can also put a label on the packaging of the flow cell to detail the date it was run, what was run on it, and for how long e.g. 13/03/2024 DDNS-run30 7 hours
If you will be storing the flow cell for future reuse, take out the bottle of Storage Buffer from the Wash Kit to thaw at room temperature.
2m
After incubation you can either follow the flow cell priming and loading steps starting from Step 19 to load a new run, or the following steps for storing the flow cell for future use.
Briefly vortex the thawed Storage Buffer to mix, then add 500μL slowly through the Priming Port.
Close the priming port before removing all waste from the waste channel. Place the flow cell back in its plastic box and envelope, then store at 4°C.
5m