BenchMark™ Protein Ladder - FAQs

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18 product FAQs found

How can you improve the transfer efficiency of the BenchMark protein ladder when Western blotting onto a PVDF membrane?

There are two factors to consider - poor transfer and the ladder passing through the membrane during the transfer.

For poor transfer onto membrane, consider:

-The percent acrylamide should be 8% to get rapid, more complete transfer of high-molecular weight proteins.

-Increase voltage, current, or length of time for transfer.

-For transfer to PVDF, omit the SDS from the transfer buffer. Addition of SDS (or use of old buffer that may have absorbed SDS leached in from the gel) will cause the proteins to bind less efficiently to PVDF membranes because it inhibits the hydrophobic interaction between the membrane and the protein.

If the problem is the protein staying in the gel, consider any of the following:

-Increase the SDS concentration to 0.1% (but use nitrocellulose).

-Eliminate the methanol in the buffer.

-Reduce the acrylamide percentage.

-Transfer longer.

If the ladder goes through membrane during transfer:

-Decrease voltage, transfer time.

-Check concentration of SDS and methanol. Too much SDS can prevent binding to membrane. Alcohol enhances hydrophobic binding to membrane; not enough alcohol may prevent binding.

-Use a 0.2 mm pore size of nitrocellulose.

-Check gel percentage; smaller proteins will pass through membranes more easily.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

What are the storage conditions and shelf life for the BenchMark Protein Ladder (Cat. No. 10747012)?

The BenchMark Protein Ladder is stable for six months if used and stored as recommended (-20 degrees C, avoid repeated freezing and thawing). We recommend aliquoting the ladder and storing it at -20 degrees C. Aliquots, once opened, should be stored at 4 degrees C.

Find additional tips, troubleshooting help, and resources within our Protein Standards and Ladders Support Center.

I used one of your protein standards for a western transfer and noticed that some of the lower-molecular weight protein bands passed through the membrane. How can I resolve this issue?

- Decrease voltage, current or length of transfer time
- Make sure that the methanol concentration in the transfer buffer is proper; use a methanol concentration of 10-20% methanol removes the SDS from SDS-protein complexes and improves the binding of protein to the membrane.
- Make sure that the SDS concentration (if added) in the transfer buffer is proper, don't use more than 0.02-0.04% SDS. Using too much SDS can prevent binding of proteins to the membrane.
- Check the pore size of the membrane and the size of the target protein. Proteins smaller than 10 kDa will easily pass through a 0.45 µm pore size membrane. If proteins smaller than 10 kDa are of interest, it would be better to use a 0.2 µm pore size membrane.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

I used one of your protein standards for a western transfer and noticed that some of the higher-molecular weight bands transferred very poorly to the membrane. Can you offer some tips?

- Increase voltage, current or length of time for transfer
- SDS in the gel and in the SDS-protein complexes promotes elution of the protein from the gels but inhibits binding of the protein to membranes. This inhibition is higher for nitrocellulose than for PVDF. For proteins that are difficult to elute from the gel such as large molecular weight proteins, a small amount of SDS may be added to the transfer buffer to improve transfer. We recommend pre-equilibrating the gel in 2X Transfer buffer (without methanol) containing 0.02-0.04% SDS for 10 minutes before assembling the sandwich and then transferring using 1X transfer buffer containing 10% methanol and 0.01%SDS.
- Methanol removes the SDS from SDS-protein complexes and improves the binding of protein to the membrane, but has some negative effects on the gel itself, leading to a decrease in transfer efficiency. It may cause a reduction in pore size, precipitation of some proteins, and some basic proteins to become positively charged or neutral. Make sure that the methanol concentration in the transfer buffer is not more than 10-20% and that high-quality, analytical grade methanol is used.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

I used one of your pre-stained standards on a Tris-Glycine gel and noticed that the molecular weights of the proteins were different than on a NuPAGE Bis-Tris gel. What is the reason for this?

Pre-stained standards have a dye that is covalently bound to each protein that will result in the standard migrating differently in different buffer systems (i.e., different gels). As a result, using a pre-stained standard for molecular weight estimation will only give the apparent molecular weight of the protein. Pre-stained standards may be used for molecular weight approximation, confirming gel migration and estimating blotting efficiency but for accurate molecular weight estimation, an unstained standard should be used.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

I used one of your protein standards and am seeing some extra bands in the lane. Can you offer some suggestions?

- While loading, take care to make sure that there is no cross-contamination from adjacent sample lanes.
- Make sure that the correct amount of standard is loaded per lane. Loading too much protein can result in extra bands and this is a problem especially with silver-stained gels.
- Improper storage of the standard or repeated freeze/thawing can result in protein degradation.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

I used one of your protein standards and the bands look non-distinct and smeary. What should I do?

Here are some suggestions:

- Make sure that the correct amount of standard is loaded per lane. Loading too much protein can cause smearing and this is a problem especially with silver stained gels.
- Bands will not be as well resolved in low percentage gels. Try using a higher percentage gel.
- If the bands look smeary and non-distinct after a western transfer/detection, this may be due to the antibody being too concentrated. Follow the manufacturer's recommended dilution or determine the optimal antibody concentration by dot-blotting.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

A couple of bands in my protein standard are missing on the gel. Can you help me troubleshoot?

Here are some suggestions:

- Check the gel type/percentage of the gel that was used. Depending on the gel type and/or percentage, all the bands may not be seen. For example, the smallest bands of the protein standard may not resolve on a very low percentage gel whereas the higher molecular weight bands may not resolve on a high percentage gel.
- Check the expiration date on the protein standard. Expired lots may result in faded or missing bands due to protein degradation.
- Check the storage conditions for the protein standard. Improper storage conditions will compromise the stability of the proteins in the standard.
- Make sure that the protein standard was not heated/boiled prior to loading on the gel. Our protein standards are ready to load and we do not recommend heating/boiling them as this may cause degradation of proteins in the standard.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

Can I use the BenchMark Unstained Protein Ladder on a NuPAGE gel?

The BenchMark Unstained Protein Ladder can be used for SDS-PAGE with NuPAGE gels, Tris Glycine gels or Tricine gels.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

Do you have the isoelectric points for the proteins in the BenchMark Unstained Protein Ladder?

Here are the isoelectric points for the proteins in the BenchMark Unstained Protein Ladder:

- 220 kDa 6.87
- 160 kDa 6.74
- 120 kDa band: 6.61
- 100 kDa band: 6.53
- 90 kDa band: 4.45
- 80 kDa band: 4.46
- 70 kDa band: 6.37
- 60 kDa band: 4.49
- 50 kDa band: 4.53
- 40 kDa band: 6.24
- 30 kDa band: 4.64
- 25 kDa band: 4.98
- 20 kDa band: 5.56
- 15 kDa band: 5.51
- 10 kDa band: 5.42


Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

What are the molecular weights of the proteins in the BenchMark Unstained Protein ladder?

The BenchMark Unstained Protein Ladder is suitable for NuPAGE, Tris-Glycine and Tricine gels. The molecular weights of the proteins in the ladder are as foll:

- Band 1: 220 kDa
- Band 2: 160 kDa
- Band 3: 120 kDa
- Band 4: 100 kDa
- Band 5: 90 kDa
- Band 6: 80 kDa
- Band 7: 70 kDa
- Band 8: 60 kDa
- Band 9: 50 kDa
- Band 10: 40 kDa
- Band 11: 30 kDa
- Band 12; 25 kDa
- Band 13: 20 kDa
- Band 14: 15 kDa
- Band 15: 10 kDa

Please note that the 20 kDa and 50 kDa bands are darker in intensity and serve as orientation bands.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

What are the origins of proteins in the BenchMark Unstained Protein Ladder?

The BenchMark Unstained Protein Ladder contain a series of affinity purified, recombinant proteins. The exact make-up and origin of each band is proprietary.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

What are the storage conditions and shelf life for the BenchMark Unstained Protein Ladder?

We recommend storing the BenchMark Unstained Protein Ladder at -20 degrees C. It may also be stored at 4 degrees C. The ladder is stable for six months when properly stored.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

Do protein standards run differently on a Zymogram gel compared to a regular Tris-Glycine gel?

Zymogram gels are essentially Tris-Glycine gels containing the substrate. Protein standards run based solely on the percentage of acrylamide and hence should run the same in both kinds of gels. It is quite possible though that if the standard is prestained, the proteins will appear a different color because of the staining (or pre-staining) of the Zymogram gels.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

Can I use any of your protein standards for estimation of protein quantity (protein quantitation)?

Our protein standards are not designed for protein quantitation.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

What is the recommended gel loading volume for your protein standards?

Please find this information in the respective manuals for the individual protein standards.

Find additional tips, troubleshooting help, and resources within our Protein Standards and Ladders Support Center.

Do I need to boil your protein standards before loading on the gel?

Our protein standards are ready to load. We do not recommend heating them as this may cause protein degradation.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.

Do I have to add reducing agent to your protein standards?

Except for our NativeMark Unstained Protein Standard (designed for native electrophoresis), all of the other unstained and prestained standards we offer (Invitrogen Sharp, SeeBlue, SeeBlue Plus2, BenchMark, HiMark) have been pre-reduced (by a proprietary method). Hence, you do not need to add reducing agent.

Find additional tips, troubleshooting help, and resources within our Protein Assays and Analysis Support Center.