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Measuring Mitochondrial Membrane Potential using the FLUOstar Omega Microplate Reader

Heather Mortiboys, Oliver Bandmann, Academic Neurology Unit, Medical School, University Of Sheffield, Beech Hill Road, Sheffield, S10 2RX, UK, 07/2008

 

  • Mitochondrial membrane potential measured in fibroblast cells
  • Tetramethylrhodamine methylester fluorescence directly proportional to the membrane potential
  • Performed on BMG LABTECH’s FLUOstar Omega in 96 and 384 well plate format

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Introduction

Measurement of the mitochondrial membrane potential is useful in a wide variety of research areas and mitochondrial dysfunction is implicated in diseases such as cancer, diabetes, Parkinson’s disease, and stroke.

In most eukaryotic cells the majority of ATP production is via oxidative phosphorylation by the respiratory chain. In this way, sugars, such as glucose, and free fatty acids are oxidised, resulting in the pumping of protons across the inner mitochondrial membrane, creating an electro-chemical gradient (the mitochondrial membrane potential). This is in turn used by the respiratory chain to generate ATP.(1) Therefore the mitochondrial membrane potential makes up a large part of the bioenergetic state of the cell and it is changed directly depending on the cells energy needs. For example fast growing tumour cells have a much higher mitochondrial membrane potential than WT cells, and in turn quiescent or differentiated cells have a still lower membrane potential.(2)

The ability to accurately measure mitochondrial membrane potential can give invaluable information about the general health and function of the mitochondria, in particular of the overall function of the respiratory chain and the potential of the mitochondria to generate ATP and provide energy for other cellular components.(3)

The number of factors which can influence this potential are vast and include many cellular components outside the mitochondria, for example interactions with the activity of the proteasome. In addition, the ability of a cell to maintain its mitochondrial membrane potential can mean the difference between survival of the cell, entry into an apoptotic cell death or a necrotic cell death process.(4) Intact mitochondrial membrane potential is also required for the cell to enter apoptosis.

Mitochondrial membrane potential is usually measured using non-invasive cationic dyes. These dyes are sequestered into the mitochondrial matrix in amounts directly proportional to the membrane potential and can then be measured using standard fluorescent techniques, including fluorescence microscopy, flow cytometry or using a microplate reader for high through put assays. BMG LABTECH’s FLUOstar Omega microplate reader was used in a high throughput screening assay measuring mitochondrial membrane potential in human cells. The results presented here were gained using primary human fibroblast cells from controls.

Materials and Methods

  • Human fibroblast cells obtained from Coriell Cell Repositories
  • Black 96 or 384 well plates with transparent bottom from Greiner (Art. No. #655090 and #781091)
  • Tetramethylrhodamine methyl ester (TMRM), Sigma #T5428
  • Carbonyl cyanide 3-chlorophenylhydrazone (CCCP), Sigma #C2759
  • Ethidium homodimer fluorescent dye, Invitrogen, #E1169
  • FLUOstar Omega microplate reader, BMG LABTECH, Offenburg, Germany (Figure 1)


Fig. 1: BMG LABTECH’s multidetection plate reader FLUOstar Omega

Fibroblasts were plated at 40% confluency in 96 or 384 well plates in minimal growth medium MEM with 10% FBS, 100 IU/mL penicillin, 100 µg/mL streptomycin, 1 mM sodium pyruvate, 2 mM L-glutamine, 0.1 mM amino acids, 50 µg/mL uridine and 1 X MEM vitamins. 24 hours later cells were changed into galactose culture medium MEM (without glucose), supplemented with 10% FBS, 100 UI/mL penicillin, 100 µg/mL streptomycin and 0.9 mg/mL galactose, as described before.(5) After further 24 hours of growth the mitochondrial membrane potential was measured using the fluorescent dye Tetramethylrhodamine methyl ester (TMRM) as described before.3 Briefly the dye was loaded onto cells at 150 nM in assay buffer (80 mM NaCl, 75 mM KCl, 25 mM D-glucose, 25 mM HEPES, pH 7.4), placed at 37°C for 5 minutes, washed 4 times in PBS and measured on a FLUOstar Omega microplate reader (Excitation: 544 nm and Emission: 590 nm, bottom reading with 50 flashes per well).

Initially TMRM is loaded into the cell via the plasma membrane and subsequently the TMRM dye is sequestered into the mitochondria as the mitochondrial matrix is the most negatively charged part of the cell. Therefore changes in plasma membrane potential could influence the results obtained using TMRM. In order to control for this, each assay is performed in parallel as above plus 10 µM carbonyl cyanide 3-chlorophenylhydrazone (CCCP), which collapses the mitochondrial membrane potential. All data is expressed as the total TMRM fluorescence minus the CCCP treated TMRM fluorescence. It is important to quantify and control for cell number, especially when comparing results between cell lines, therefore cell number is measured using 1 µM ethidium homodimer fluorescent dye in a parallel plate after freeze thawing (Excitation: 544 nm and Emission: 645 nm, bottom reading with 50 flashes per well).

Results and Discussion

Figure 2 shows the mitochondrial membrane potential in 6 control fibroblast cell lines, each measured in triplicate on separate occasions and showing the lack of variation between control cell lines.


Fig. 2: Mitochondrial Membrane Potential measured using TMRM fluorescence in 6 different control fibroblast lines. The fluorescence values were corrected for the cell number.

Figure 3 shows the reduction in membrane potential of the same control fibroblasts after treatment with mitochondrial toxin ‘X’ for 72 hours. This demonstrates the range at which the assay is sensitive, creating a large ‘therapeutic window’. Also in this figure the control cells have been treated with an experimental compound ‘Y’ which rescues the reduction in mitochondrial membrane potential caused by treatment with the mitochondrial toxin ‘X’.


Fig. 3: Comparison of mitochondrial membrane potential in 6 untreated control fibroblast lines (norm), treated with mitochondrial toxin X alone and treated with mitochondrial toxin X and rescues compound Y. The fluorescence values obtained measuring TMRM were corrected for the cell number.

Figure 4 shows that the assay can reliably be scaled up to a 384 well plate format and gain robust, reproducible results.


Fig. 4: Fluorescence intensity values indicating the membrane potential in control fibroblast in 384 well plate (192 wells used). The values were obtained either after treatment with mitochontrial toxin X alone or mitochondrial toxin X and rescue compound Y.

Conclusion

These results show that the FLUOstar Omega is suitable for measuring mitochondrial membrane potential in both 96 and 384 well plate formats. In addition, prolonged low dose treatment of healthy control fibroblast with a mitochondrial toxin causes a significant reduction in mitochondrial membrane potential.
The results are reproducible across a number of different control fibroblast lines and the results of the rescue of this defect with the experimental compound provide further evidence that this assay can be used for high throughput screening using BMG LABTECH’s FLUOstar Omega.

References

  1. Adam-Vizi V (2005) Production of reactive oxygen species in brain mitochondria: contribution by electron transport chain and non-electron transport chain sources. Antioxid. Redox Signaling 7 (9-10), 1140-1149.
  2. Huang SG. (2002) Development of a high throughput screening assay for mitochondrial membrane potential in living cells. J. Biomol. Screen. 7, 383-389.
  3. Brown GC (1999) Nitric Oxide and Mitochondrial Respiration. Biochim. Biophys. Acta 1411 (2-3), 251-269.
  4. Carelli V, Rugolo M, Sgarbi G, Ghelli A, Zanna C, Baracca A, Lenaz G, Napoli E, Martinuzzi A, Solaini G (2004) Bioenergetics shapes cellular death pathways in Leber’s hereditary optic neuropathy: a model of mitochondrial neurodegeneration. Biochim. Biophys. Acta 1658, 172– 179.
  5. Hofhaus G, Johns DR, Hurko O et al. (1996) Respiration and growth defects in transmitochondrial cell lines carrying the 11778 mutation associated with Leber’s hereditary optic neuropathy. J. Biol. Chem. 271, 13155-13161.