A Step-by-Step Guide to Designing qPCR Primers
Quantitative PCR (qPCR) primer design is a critical step when setting up your qPCR or reverse transcription-qPCR assay (RT-qPCR) for gene expression analysis. qPCR primers that anneal poorly or that anneal to more than one sequence during amplification can significantly impact the quality and reliability of your results.
Also, if you are performing a one-step reverse transcription PCR (RT-qPCR), the reverse transcriptase will use the reverse primer to prime the transcription reaction. In this scenario, a poor primer would result in both inefficient reverse transcription and inefficient amplification – a lose–lose situation.
Considering the above, it’s well worth spending the time necessary to design good-quality qPCR primers. This article will tell you exactly how to do that!
The good news is that primers are cheap, so you can easily test several different pairs to choose the best ones for your experiment.
The bad news is that primer testing requires time and patience, so the sooner you get a pair of primers working, the better.
The NCBI tool Primer-BLAST is widely used for qPCR primer design. There are many other primer design tools available online, including primer3, and PCR suppliers often offer their own design programs free of charge.
Below are the main steps involved in qPCR primer design using the NCBI tool Primer-BLAST.
The design steps will be similar if you use other primer design programs, and the information below should give you an idea of the parameters to watch out for.
qPCR Primer Design: Getting Started
The first step in designing primers is to get the nucleotide sequence of your gene of interest.
Go to the Pubmed gene database and search for your gene of interest. You can then filter by species in the right-hand corner of the next screen.
Click on your gene of interest and scroll down until you find the NCBI Reference Sequence (RefSeq) for your gene (e.g. “NM_203483”). Note that there may be multiple sequences if your gene has different isoforms – make sure you click on the isoform you are interested in.
Click on the name and on the next screen, you will see a link to “Pick primers” in the right-hand corner of the screen underneath “Analyze this sequence”. Click on this link to take you to the Primer-BLAST tool.
The Primer-BLAST tool has many parameters and options to set. The next sections take you through each of the options in the tool and explains what to set for each one and why.
Parameters for qPCR Primers
This section covers some of the basic settings for your primers, including the PCR product size and melting temperature. There is also an option to include sequences for reverse or forward primers.
Set the following primer parameters:
- PCR product/amplicon size: For efficient amplification, design the primers so that the amplicon is between 70 and 200 bp long.
- Number of primers to return: This is up to you, depending on how many options you want to choose from. It won’t take long for the program to design 10 primer pairs, and this should give you a reasonable chance of finding a suitable pair.
- Melting temperature: As a rule, aim for a minimum of 60°C and a maximum of 63°C; the ideal primer melting temperature is 60°C (with a maximum difference of 3°C in the melting temperatures, Tm, of the two primers). You can use a Tm calculator to determine these temperatures.
To avoid amplification of contaminating genomic DNA, design primers so that one-half of the primer hybridizes to the 3′ end of one exon, and the other half to the 5′ end of the adjacent exon.
To do this, simply select “Primer must span an exon–exon junction.” You don’t need to change the other settings.
Primer pair specificity checking parameters
Use the default settings. The program will use the RefSeq mRNA sequence from the organism you selected to design the primers.
Checking the Output Screen
Once all the parameters are set, clicking on ‘Get primers’ returns a list of potential forward and reverse primer sequences to choose from. This can take a while but the screen updates periodically to show the time since submission.
Take a look at the options the program returned and pay special attention to the following:
- Make sure the 3′ end of the primer contains a C or G residue because T and A residues bind more easily to DNA in a non-specific way.
- Aim for a GC content of around 40–60% to ensure maximum product stability.
- Avoid self-complementarity to decrease the possibility of primer–dimer formation. Ideally, the primer should have a near-random mix of nucleotides.
Now, pick the best two or three primers, order and test them. Good luck!
If you have any other top tips for qPCR primer design, we’d love to hear from you in the comments!
Need help in other areas of qPCR from setup to data analysis? Check out our top 11 qPCR papers every researcher should know.
Need help making your PCR fail (a bit) less often? Download our free notorious PCR inhibitors poster and pin it up near your DNA engine. Or download the Bitesize Bio PCR eBook for more comprehensive practical guidance.
Originally published February 6, 2013. Reviewed and republished 2017 and April 2021.
It is crucial to reflect monovalent cation, Mg2+, and dNTPs concentrattion in the Tm calculation and to check the potential primer dimers. A suitable online application is Primer Inspector at http://www.molbiotools.com/primerinspector.php
When I try to use the method you suggested, it tells me that my template is too long, and to select a ‘from’ for my forward primer and a ‘to’ for my reverse. Isn’t the whole point of the program to find a good ‘from’ and ‘to’ point, in order to match my requirements (PCR product size, spaniing an exon-exon junction, etc)
I’ve limited my pcr product size to 100-200bp, so I don’t quite see how the template is too large. Am I missing something?
I would like to design random primers which can amplified just whole genome of bacteria, what could I do? Could you help me, please!