Staining proteins following SDS-PAGE or 2-dimensional electrophoresis is necessary for visualizing a global population of proteins or checking the expression of your recombinant proteins.

But how do you know which protein staining method to use?

This article explains the pros and cons of three of the most common protein staining methods: silver staining, coomassie brilliant blue staining, and InstantBlue staining.

1. Silver Stain

Need a high sensitivity stain with no requirement for downstream applications? Silver staining may just be what you need.

How Does It Work?

Silver staining exploits the silver cation (Ag1+) binding capacity of proteins. The silver cations bind to the target protein(s) and are subsequently reduced to silver metal using a developing solution. This creates a visible image.

Pros and Cons

The primary benefit of silver staining is its high sensitivity (see below). However, silver staining involves multiple steps and reagents, making the process relatively time-consuming and laborious.

In addition, the gel requires developing after staining, in order to visualize the proteins, and the length of time required for developing is highly variable between gels. The upshot of this is low reproducibility.

Another disadvantage of silver staining is that the use of formaldehyde when fixing the gel makes silver staining incompatible with mass spectrometry. Silver staining protocols do exist that are compatible with mass spectrometry but at the sacrifice of sensitivity.

Silver staining also has a narrow linear dynamic range (the range at which the level of staining is directly proportional to protein concentration), making it less suitable for quantification.

Approximate Limit of Detection

Silver staining can detect ~ 1 ng of protein [1] which makes it extremely useful for applications involving low protein levels.

A Researcher’s Opinion

Silver staining is my least favorite of the protein staining methods, not just because of the multiple steps required but also due to the use of several dangerous chemicals (including silver nitrate and formaldehyde), which I like to avoid if possible. It’s also really difficult (from my experience) to remove silver stains from benches and equipment—so beware!

If you want more information on and protocols for different silver protein staining methods, including those for use with mass spectrometry, check out this paper by Chevallet et al. [2]

2. Coomassie Brilliant Blue

Coomassie staining is probably the most well-known protein staining technique. Two main types of coomassie staining exist:

Let’s discuss them in that order.

Classical Coomassie

Need a reliable, bread and butter protein staining method that you can share with your lab group? Classical coomassie protein stain is the way forwards.

How Does It Work?

The classical coomassie protein staining technique involves incubating the gels with a coomassie staining solution. This stains the entire gel, not just the proteins. The stain is subsequently removed by agitating the gel in a solution of 10% acetic acid, 50% methanol, and 40% H2O. This process is called destaining.

Because the dye is retained better by the protein molecules than the porous gel matrix, the protein bands become visible.

Pros and Cons

The classical coomassie protein staining method is cheap and easy, but is considerably less sensitive than silver staining, making visualization of low abundance proteins difficult. The low reproducibility of classical coomassie staining is also a disadvantage due to the difficulty in standardizing the destaining step.

One big advantage of coomassie staining is that it is compatible with mass spectrometry.

Approximate Limit of Detection

Classical coomassie has a lower limit of detection of ~ 100 ng. [1]

A Researcher’s Opinion

This protein staining method is my personal favorite for simple tasks such as visualization of recombinant proteins, or generated antibodies, as it’s simple and quick to perform. This makes it great for day-to-day use.

Colloidal Coomassie

Colloidal coomassie protein stain provides a happy medium between classical coomassie staining and silver staining, having relatively high sensitivity and being simple to perform. It’s also compatible with protein mass spectrometry.

How Does It Work?

This method is an adaptation of classical coomassie staining that uses a modified coomassie dye (G-250 instead of R-250). Fancy a game of spot the difference? The structures of G-250 and R-250 are shown in Figure 1 below.

Because the colloidal dye does not penetrate the gel, no destaining is required. Destaining may be performed, however, to increase the contrast between the protein bands and the background.

Pros and Cons

Colloidal coomassie has several advantages over classical coomassie protein staining. These include increased sensitivity and higher reproducibility than silver and classical coomassie staining due to the absent destaining step.

All good things come at a cost, however, and colloidal coomassie kits will cost you a bit more than your regular coomassie stain.

Many protocols for protein staining using colloidal coomassie are available, several of which are described and compared in this paper by Dyballa and Metzger. [3]

Approximate Limit of Detection

Colloidal coomassie has a detection limit of ~ 10 ng, making it about an order of magnitude more sensitive than classical coomassie.

A Researcher’s Opinion

The increased sensitivity of this protein staining method over classical coomassie makes it great for experiments involving low protein levels, such as analyzing binding proteins in co-IPs, especially when you’re considering quantifying the protein bands using mass spectrometry.

Protein Staining Methods: An Overview of 3 of the Best
Figure 1. The structures of coomassie (G-250) and colloidal coomassie (R-250). (Image credit: Thomas Warwick.)

3. InstantBlue™

In a rush? Or simply can’t be bothered with all that staining and destaining malarkey? Thank goodness for InstantBlue™.

It’s another coomassie-based protein stain but formulated in such a way to provide one-step visualization of your proteins.

How Does It Work?

I’d love to be able to tell you how this protein staining method works, but that big registered trademark symbol means there’s a bit of an information vacuum.

The user manually cryptically states “InstantBlue contains Coomassie [sic] dye, ethanol, phosphoric acid and solubilizing agents in water”.

Given that no destaining is required, it must act similarly to colloidal coomassie and stain specifically protein molecules and not the gel.

Pros and Cons

InstantBlue™ protein stain works fast. Very fast. You’ll see your protein bands in 10–15 minutes. Being a one-step procedure, it’s also quick and reproducible. And like the other coomassie-based stains it’s fully compatible with mass spectrometry.

It’s photosensitive, however, and will degrade over time. You can re-use it, but siphon off the re-used stuff into a separate opaque container and discard it when you notice it’s no longer staining your proteins.

Approximate Limit of Detection

InstantBlue™ protein stain can detect proteins down to ~ 5 ng. If you’re struggling to see faint protein bands, soak your developed gel in water to increase their contrast.

A Researcher’s Opinion

When I’m purifying proteins for X-ray crystallography, I don’t have the time to wait for my gels to destain before I can be sure I’ve actually expressed my target. That’s why I use the InstantBlue™ protein staining method. The only problem is other lab users steal it, so keep your own secret stash.

A Recap of the Protein Staining Methods Discussed

It wouldn’t be a great article if it wasn’t information-dense! Here’s a summary of the different protein staining methods presented above.

Table 1. A summary of silver, coomassie, colloidal coomassie, and InstantBlue™ stains.

[table id=185 /]

Hopefully, you’re now armed with enough information to choose the protein staining method that’s most appropriate for your intended experiments.

Has this article on protein staining methods been a boon? Have we missed some salient facts out? Be sure to let us know in the comments section below!

Originally written and published September 2012 by Laura Grassie. Reviewed and updated January 2022 by Thomas Warwick.


  1. Weiss W et al. (2009) Protein detection and quantitation technologies for gel-based proteome analysis. Methods Mol Biol 564:59–82
  2. Chevallet M, Luche S, and Rabilloud T (2006) Silver staining of proteins in polyacrylamide gels. Nat Protoc 1:1852–1858
  3. Dyballa N and Metzger S (2012) Fast and sensitive coomassie staining in quantitative proteomics. Methods Mol Biol 893:47-59

More 'Protein Expression and Analysis' articles


  1. Yes, what Min has said about microwaving your gel is right. It helps you save a lot of time but you have to be careful so that you don’t overheat the gel or it might dehydrate, other than that it has no detrimental effect on the gel.

    And also you can do chloroform staining prior to coomasie staining if you have tryptophan residues in your protein, as chloroform binds to tryptophan and fluoresces under UV light. So it can be used as initial screening of your protein bands. You just have to soak the gel in chloroform for 1 min wash it MQ water until the chloroform is removed and then view it under UV light.

  2. Great article Laura. I just wanted to pitch-in a little bit more information here and there. First, regarding the colloidal Coomassie staining, there is a method dubbed “blue silver” by Giovanni Candiano published in the journal of Electrophoresis (2004) 25 1327-1333 that has a sensitivity in the 1 ng range and is less time consuming than you alluded to. With this method, I get perfectly stained gels in just 4 hrs (3 x 10 min for washing gels in MQ water, 3 h staining with the “blue silver”, 30 min destaining with MQ water). Second, the classical Coomassie staining can be accelerated by microwaving the gel until the stain or destain solution just begins to boil and let the gel rock at RT for 5 min, each time. Just a few tips.

    1. Thanks for that extra info Min! I didn’t know you could microwave your gel, does it ever have a detrimental effect on the gel or any downstream applications?

  3. Thank you for the very interesting post. You didn’t touch on “Ponceau S” staining which I really like for checking complete transfer of WB, and to a lesser extent to detect equal loading of protein samples.

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