Split-root systems are widely studied and have been adapted to rhizoboxes as well as to pots and tubes . In the rhizosphere, plants host a wide diversity of bacteria on the surface of the root as well as within roots in the vascular tissue . Due to its abundance and importance, the bacterial community in the rhizosphere is perhaps the most widely studied among other microbial members in the rhizosphere ecosystem. While the study of endophytic bacteria requires inevitable destructive sampling due to its localization, several non-destructive approaches have been developed to study microbes inhabiting the rhizoplane. One of the most widely studied plant-microbe interactions in the rhizosphere is that of the symbiotic relationship between legumes and rhizobia . Once a potential nodule forming bacteria is isolated, it is often required to authenticate its nodule forming phenotype by inoculating on host plants. However, conventional methods such as the use of soil pouches do not allow long term incubation, while “Leonard jars,” consisting of two stacked glass jars forming the top soil layer and the bottom nutrient solution layer, can be expensive and time consuming . A recent study challenges this by describing the use of clear plastic CD cases as minirhizotrons with potential for use in phenotyping root traits such as legume formation, and demonstrated innovation that democratizes research opportunities in rhizosphere research . Other microbial interactions in the rhizosphere, however, may not result in visible changes to the root system and often rely on next-generation omics technologies. As such,macetas plastico physical separation of the rhizosphere from the bulk soil becomes paramount in elucidating changes to microbial community and interactions.
One approach to this end is the use of nylon bags with differing pore sizes . The nylon bag restricts the movement of roots and the soil inside the bag is then regarded as the rhizosphere soil to compare against the surrounding root free bulk soil . Developing further on this concept, Wei et al. designed a specialized rhizobox that allowed repeated non-destructive sampling by adding individual nylon bags of root-free soil surrounding the root compartment which are then used as a proxy for the rhizosphere . These methods allowed easy distinction of the rhizosphere and the bulk soil but, we now know that the rhizosphere community is not only distinct from the bulk soil but also varies with type, part and age of the root, largely as a consequence of varying root exudation patterns . Studying this phenomenon in situ in the soil requires separation of desired roots from others without disturbance to plant growth or soil. To address this, researchers have used a modified rhizobox design with a side compartment to regulate root growth and quarantine specific roots from the main plant chamber . This additionally creates easy distinction between old and new roots and allows testing on specific quarantined roots despite plant age. A study using this set up showed specific microbial chemotaxis toward different exudates on an individual root whereas another showed spatial and temporal regulation of niche differentiation in microbial rhizosphere guilds . Similar physical perturbations to regulate root growth in response to microbial stimuli have also been applied in the micro-scale and are explored in the next section. Our assessment of the major growth chambers showed that most of the systems applied share similarities in basic structural components such as in the use of two parallel sheets in rhizoboxbased devices. While these growth chambers brought many of the rhizosphere processes to light, limitations do exist. One limitation is with the scale of applicability.
Most of these growth systems are mesoscale and can easily reproduce pot scale studies but may not be easily translatable to interactions occurring at the micro-scale nor recapitulate processes occurring at field-relevant scale. The next section describes advances in technology resulting in a new wave of unique devices making use of microfluidic processes and fabricated ecosystems which are specifically made to investigate specific rhizosphere processes. A complex web of biochemical processes and interactions occur in micro-scale dimensions in the rhizosphere. Having the ability to interrogate and manipulate these micro-scale processes and environmental conditions with high spatiotemporal resolution will elucidate mechanistic understanding of the processes. Microfluidics has proven to be a powerful approach to minimize reagent usage and to automate the often-repetitive steps. The micro-scale of the channels also allows precise control of reproducible conditions utilizing the laminar flow and automated fluidic operations . In addition, the microfluidic devices are well integrated with conventional imaging techniques by using a glass slide or coverslip as a substrate bonded with polydimethylsiloxane . These characteristics, as well as the ability to rapidly prototype and reproducibly manufacture using soft lithography technique, have enabled new ways of interrogating and studying the rhizosphere environment in a reproducible manner. Many of the microfluidic devices used for studying the rhizosphere share a similar design concept . They have an opening port, sometimes with pipette tips inserted into the PDMS body where the seed of the seedling rests and a micro-channel where the primary root grows into.
For example, an Arabidopsis thaliana’s seedling is typically grown in a microfluidic device up to 10 days, with chamber dimension around 150 to 200 µm in height, whereas the Brachypodium distachyon seedling chamber is 1 mm in height due to its thicker roots . Media and/or inoculation of the microbiome is achieved through additional channels to the main chamber. The PDMS body with the channels is typically bonded on a 50 mm by 75 mm microscope slide, and is made to accommodate multiple plants to increase throughput. Automated control offers the ability for continuous imaging and manipulation of media conditions with high temporal resolution. One notable example of a microfluidic device for rhizosphere studies is the RootChip, which uses the micro-valves in a PDMS device to control the fluidics . The first study using the RootChip grew 8 Arabidopsis plants on a single device with micro-valves but by the second iteration, the throughput has been doubled indicating rapid technological advances in the field. In addition, all these studies demonstrated spatiotemporal imaging at single-cell resolution and dynamic control of the abiotic environments in the rhizosphere. Another microfluidics-specific application to rhizosphere study is to use the laminar flow to generate the spatially precise and distinct micro-environment to a section of the root as demonstrated by Meier et al. . A young Arabidopsis’ seedling was sandwiched and clamped between two layers of PDMS slabs with microchannel features to tightly control synthetic plant hormone flow with 10 to 800 µm resolution to the root tip area,cultivar arandanos enabling observations of root tissues’ response to the hormones. As many root bacteria produce auxin to stimulate the interactions with the root, this study showed the possible mechanism of microbiome inducing the interaction by stimulating root hair growth. Another application of laminar flow utilized the RootChip architecture by adding the two flanking input channels to generate two co-laminar flows in the root chamber, subjecting a root to two different environmental conditions along the axial direction to study root cells adaptation to the micro-environment at a local level . These studies revealed locally asymmetrical growth and gene pattern regulations in Arabidopsis root in response to different environmental stimuli. Microfluidic platforms have also been successfully employed to study the interactions between the root, microbiome and nematodes in real time . In the systems, additional vertical side channels are connected perpendicularly to the main microchannel to enable introduction of microorganisms and solutes to the roots in a spatially and temporally defined manner . A recent micro-fluidic design incorporated a nano-porous interface which confines the root in place while enabling metabolite sampling from different parts of the root . These studies demonstrated the potential of microfluidics in achieving spatiotemporal insights into the complex interaction networks in the rhizosphere. Despite several advantages of microfluidics in rhizosphere research as described above, some challenges remain. All the microfluidic applications grow plants in hydroponic systems where clear media is necessary for the imaging applications and packing solid substrates in the micro-channels is not trivial.
The micro-scale of the channels limits the applications of these devices to young seedlings. Thus, interrogating the micro-scale interactions in bigger, more developed plants is not possible with current microfluidic channel configurations. In addition, technical challenges such as operating the micro-valves and microfabrication present a barrier to device design and construction for non-specialists. Fabricated ecosystems aim to capture critical aspects of ecosystem dynamics within highly controlled laboratory environments . They hold promise in accelerating the translation of lab-based studies to field applications and advance science from correlative and observational insights to mechanistic understanding. Pilot scale enclosed ecosystem chambers such as EcoPODs, EcoTrons and EcoCELLs have been developed for such a purpose . These state-of-the-art systems offer the ability to manipulate many parameters such as temperature, humidity, gas composition, etc., to mimic field conditions and are equipped with multiple analytical instruments to link below ground rhizosphere processes to above ground observations and vice versa . Currently, however, accessibility to such systems is low as there are only several places in the world which can host such multifaceted facilities due to the requirement of significant financial investments. Switching back to lab-scale systems, a recent perspective paper calls for the need to standardize devices, microbiomes and laboratory techniques to create model ecosystems to enable elucidation of molecular mechanisms mediating observed plant-microbe interactions e.g., exudate driven bacterial recruitment . Toward this goal, open source 3D printable chambers, termed Ecosystem Fabrication devices, have been released with detailed protocols to provide controlled laboratory habitats aimed at promoting mechanistic studies of plant-microbe interactions . Similar to a rhizotron setup, these flow through systems are designed to provide clear visual access to the rhizosphere with filexibility of use with either soil or liquid substrates . Certainly, there are many limitations to these devices in that they are limited to relatively small plants and limit the 3D architecture of the root system. Still, an advantage with the EcoFAB is that its 3D printable nature allows for adaptations and modifications to be made and shared on public data plat forms such as Github for ease of standardization across different labs and experiments . In fact, a recent multilab effort showed high reproducibility of root physiological and morphological traits in EcoFAB-grown Brachypodium distachyon plants . The development of comparable datasets through the use of standardized systems is crucial to advancing our understanding of complex rhizosphere interactions. Open science programs such as the EcoFAB foster a transparent and collaborative network in an increasingly multidisciplinary scientific community. Specialized plant chamber systems are necessary for nondestructive visualization of rhizosphere processes and interactions as all destructive sampling approaches tend to overestimate the rhizosphere extent by 3–5 times compared to those based on visualization techniques . Nonetheless, plants in such chambers are still grown in defined boundaries and suffer from inherent container impacts. For instance, studies have pointed out that container design significantly influences root growth during early developmental stages and leaves lasting impacts on plant health and phenotype . The majority of the lab-based chambers are also centimeter scale and are unlikely to replicate exact field conditions in terms of soil structure, water distribution, redox potential or root zone temperatures . While comparisons between chamber-grown and pot-grown plants show similar outputs , studies comparing plants grown in confined spaces to those directly grown in the field are missing. A recent review mapped the gradient boundaries for different rhizosphere aspects and found that despite the dynamic nature of each trait, the rhizosphere size and shape exist in a quasi-stationary state due to the opposing directions of their formation processes . The generalized rhizosphere boundaries were deducted to be within 0.5–4 mm for most rhizosphere processes except for gases which exceeds > 4 mm and interestingly, they are independent of plant type, root type, age or soil . Bearing this in mind, our assessment of the different growth chambers revealed possible overestimation of rhizosphere ranges in some chamber set ups. For instance, the use of root-free soil pouches representing rhizosphere soil despite being cm-distance away from the rhizoplane. This prompts the need for careful evaluation of new growth chamber designs to ensure accurate simulation of natural rhizosphere conditions.