Quantitative Analysis of Plasmodesmata Permeability using Cultured Tobacco BY-2 Cells Entrapped in Microfluidic Chips
Plasmodesmata are unique channel structures in plants that link the fluid cytoplasm between adjacent cells. Plants have evolved these microchannels to allow trafficking of nutritious substances as well as signaling molecules for intercellular communication. However, tracking the behavior of plasmodesmata in real time is difficult because they are located inside tissues. Hence, we developed a microfluidic device that traps cultured cells and fixes their positions to allow testing of plasmodesmata permeability. The device has 112 tandemly aligned trap zones in the flow channel. Cells of the tobacco line BY-2 were cultured for 7 days and filtered using a sieve and a cell strainer before use to isolate short cell clusters consisting of only a few cells. The isolated cells were introduced into the flow channel, resulting in entrapment of cell clusters at 25 out of 112 trap zones (22.3%). Plasmodesmata permeability was tested from 1 to 4 days after trapping the cells. During this period, the cell numbers increased through cell division. Fluorescence recovery after photobleaching experiments using a transgenic marker line expressing nuclear-localized H2B-GFP demonstrated that cell-to-cell movement of H2B-GFP protein occurred within 200 min of photobleaching. The transport of H2B-GFP protein was not observed when sodium chloride, a compound known to cause plasmodesmata closure, was present in the microfluid channel. Thus, this microfluidic device and one-dimensional plant cell samples allowed us to observe plasmodesmata behavior in real time under controllable conditions.