Sample requirements for Sequencing – Sanger

Sample requirements and sample analysis

Preparation of samples


We need 5µl per reaction of both your primer and DNA at the concentrations specified below

Plasmid DNA 100ng/µl
PCR product 1ng/µl per 100bp
Bacterial culture 1ml of overnight culture
Primers 3.2pmol/µl

DNA concentration needed

  • Plasmid: We require a concentration of 100ng/ul for plasmid samples.
  • Purified PCR samples: The concentration of DNA required is dependent on the length of the sample sent. A concentration of 1ng/ul per 100 base pairs is required for successful sequencing.


We require your primers to be sent at 3.2pmol/ul and we require 5µl per reaction. You can choose to send your own primers, use our stock primers or you can order custom primers that will be delivered to the sequencing laboratory. It is recommended when designing primers that you ensure you pick a suitable primer length of between 18 and 23 base pairs long, design your primers at least 50 bases upstream of your area of interest, a tm between 55°C and 60°C and ensure your primer has a GC content between 40 and 60%.

Quality of samples

All samples must be of a good quality, free from contaminants such as salts, other contaminating DNA, unincorporated dinucleotides (in PCR reactions) and other reagents that would interfere with the reaction.

It would be advisable to run your samples on agarose gels prior to submission to ensure that only one clearly defined band is visible on the gel and your DNA is not contaminated with other DNA and has not degraded.

It is important that you are aware of any motifs or secondary structures that might impede high quality sequencing results. If you know that this is most likely going to be a problem we recommend you use our secondary structure resolution option when ordering.

Receiving results

In order to receive your results as soon as possible it is advisable that you choose our free SpeedREAD™ service. SpeedREAD™ is an automatic service which dispatches your results as soon as the sequencer has completed the analysis. If you choose this option you will receive an automatic email with a link to your results. This will be followed up with an email from our sequencing team the following working day. This email will include the results of their quality checks on your samples and if your samples did fail the sequencing team will advise you as to why they failed and potential solutions.

What good sequencing traces look like

Below (Figure 1 and Figure 2) are examples of good sequencing traces of a high quality. Figure 1 displays a plasmid sample which has produced a good sequencing trace.  Figure 2 is of a PCR sample, PCR samples produce peaks of equal height the whole way through the sequence. This raw data gives us information on the length of the read and the height of the peaks which determines whether or not the peaks are within acceptable heights.  Figure 3 is an electropherogram for a good quality sequencing trace. Note it has well defined peak resolution, uniform peak spacing and has a weak background noise in comparison to the sample.

Good Sequencing Read

Figure 1 – Raw data for a plasmid sample which gives a good quality sampling trace

Raw Data For PCR Sample

Figure 2 – Raw data for a PCR sample which gives a good quality sequencing trace


Figure 3 – Electropherogram for a sample which gives a good quality sequencing trace

Most common reasons why sequencing reactions fail

Samples too concentrated

Figure 4 is the raw data from a PCR product that was too concentrated. As shown in the figure the results reach above the highest detectable levels on the graph. Figure 5 is the corresponding electropherogram for this sample. Note the peaks are poorly defined, overlap and are not uniformly spaced. The sample produced what would be known as a mixed trace, this would be due to the poorly resolved base calling in the electropherogram. Figure 6 shows a plasmid sample which is too concentrated, the sequencing trace is very concentrated at the beginning and it decreases rapidly producing a shorter than expected sequencing trace.

Raw Data For PCR Sample Too Concentrated

Figure 4 – Raw data for a PCR sample which is too concentrated

Electropherogram Too Concentrated

Figure 5 – Electropherogram for PCR reaction which is too concentrated

Raw Data For Plasmid Sample Too Concentrated

Figure 6 – Raw data for a plasmid sample which is too concentrated

Low sequencing trace

Figure 7 and Figure 9 display failed sequencing traces. On the raw data (Figure 7) the scale is low and there is no obvious increase in fluorescence. Figure 8 shows the electropherogram for data from Figure 7 no bases are called and they are all assigned with the letter N. In Figure 9 the sample has failed due to a low concentration of DNA in the sample, there is some binding but at a low level of fluorescence. Figure 10 is the electropherogram for Figure 9, bases are not being called with a high quality of confidence.

Raw Data For A Sample Which Has Not Produced Any Results

Figure 7 – Raw data for a sample that has not produced any results

Figure 8

Figure 8 – Electropherogram for sample which has not produced a sequencing trace

Figure 9

Figure 9 – PCR sample which has failed due to a low concentration of DNA in the sample

Figure 10

Figure 10 – Electropherogram for PCR sample which has produced a low fluorescence

Table 1: Potential causes for samples producing a poor sequencing trace
Probable cause Solution
Insufficient DNA concentration Increase DNA concentration
Insufficient primer binding Redesign primer
No primer binding site present Redesign primer or use different primer
Degraded DNA Re-extract DNA template or clean up template
Degraded primer Make up new primer stock

Secondary structures

Secondary structures are unexpected early terminations of your sequence (Figure 11). These can be due to your template having a high number of GC rich areas which have a tendency of causing the DNA to loop to form a hairpin bend. They polymerase cannot continue the reaction and therefore the sequence terminates early.

Figure 11

Figure 11 – Figure of a secondary structure. The arrow shows where signal is lost due to the secondary structure

Table 2: Potential causes for early termination of a sequencing trace
Probable cause Solution
Secondary structure present in your DNA Choose secondary structure resolution option when ordering
Redesign primers to avoid the formation of the secondary structure

Mixed traces

Several different mixed traces can be produced dependent on why the sample has produced a mixed trace. If the trace has produced a mixed trace the whole way through the electropherogram (Figure 12) it is most likely due to either your sample containing more than one DNA template or your primer binding to more than one area of on your DNA.

Other mixed traces that could be produced could be due to mutations in your template. Single nucleotide polymorphisms (SNP) could cause what would look like a mixed trace at one particular base which does not affect the rest of the sequencing trace (Figure 13). An insertion or deletion in the DNA however will look like a normal sequence until the insertion or deletion occurs and then a mixed trace will occur as different sequences are now being produced. A mixed trace might occur due to enzyme slippage also, this can occur after a homopolymeric region (Figure 14), this enzyme slippage happens and the growing strand does not stay paired correctly with the template DNA during polymerization.

Figure 12

Figure 12 – Electropherogram showing a mixed trace

Figure 13

Figure 13 – Electropherogram showing SNPs

Figure 14

Figure 14 – Electropherogram showing enzyme slippage following a homopolymeric region

Table 3: Potential causes of mixed sequencing traces
Probable cause Solution
Mixed templates present in sample Re-isolate DNA
Frame shift mutation Use different primer after the mutation or sequence the complimentary strand
Multiple primer binding sites Ensure the primer will only bind at one spot
Enzyme slippage due to a homopolymeric region Sequence the complimentary strand

Dye Blobs

Unincorporated dye terminators (commonly called “Dye Blobs”) appear at positions 70 to 80bp and again at approximately 100bp. The chromatogram below shows unincorporated dye-terminators superimposed over and partially obscuring the real peaks.

Dye Blobs

Dye blobs are caused by an imbalance of primer:BigDye:template. We use proprietary clean-up plates to remove dye blobs but in extreme cases of imbalance they can still remain. We have optimised primer:BigDye concentrations for specified template concentrations and so it is important that you work to send the correct template concentration if you find that Dye Blobs are a problem for you.


Leave a Reply

Fill in your details below or click an icon to log in: Logo

You are commenting using your account. Log Out /  Change )

Google+ photo

You are commenting using your Google+ account. Log Out /  Change )

Twitter picture

You are commenting using your Twitter account. Log Out /  Change )

Facebook photo

You are commenting using your Facebook account. Log Out /  Change )


Connecting to %s