Spatial organization in microbial range expansion emerges from trophic dependencies and successful lineages


Evidence suggests that bacterial community spatial organization affects their ecological function, yet details of the mechanisms that promote spatial patterns remain difficult to resolve experimentally. In contrast to bacterial communities in liquid cultures, surface-attached range expansion fosters genetic segregation of the growing population with preferential access to nutrients and reduced mechanical restrictions for cells at the expanding periphery. Here we elucidate how localized conditions in cross-feeding bacterial communities shape community spatial organization. We combine experiments with an individual based mathematical model to resolve how trophic dependencies affect localized growth rates and nucleate successful cell lineages. The model tracks individual cell lineages and attributes these with trophic dependencies that promote counterintuitive reproductive advantages and result in lasting influences on the community structure, and potentially, on its functioning. We examine persistence of lucky lineages in structured habitats where expansion is interrupted by physical obstacles to gain insights into patterns in porous domains.


Bacterial life in natural environments is predominantly associated with sessile assemblages of cells that form aggregates or surface-attached biofilms1,2,3,4,5. The confinement of bacterial cells in sessile colonies and their limited relocation opportunities makes positioning in space a critical factor for access to nutrients6, exchange of metabolites7, protection from phage infection8, or protection from predation9. Within such highly constrained systems, scenarios emerge in which a few cells contribute disproportionally to the long term community biomass10 supporting the notion of “survival of the luckiest”. Evidence in the form of genetic segregation of initially mixed communities is observed frequently in colonies growing on surfaces11,12,13,14,15,16,17,18, or observations of detrimental mutations accumulating at the assemblage periphery that are rapidly lost in homogeneous environments such as liquid cultures19. During sessile growth, bacterial cells are essentially fixed in space and depend on diffusional fluxes dictated by heterogeneous nutrient landscapes (governed by the surface and their neighbors) that ultimately shape the resulting bacterial assemblage6. In contrast to advection dominated planktonic life style, bacterial cells in diffusion dominated systems often self-engineer their immediate surroundings (a process frequently termed niche construction20). For example, single species biofilms engage in cross-feeding interactions through divergent behavior of spatially segregated subpopulations experiencing fundamentally different growth conditions21,22. Overall, trophic interactions have the potential to shape the emerging community patterns during bacterial range expansion. When competing for the same resource, the front of an expanding population offers advantages due to preferential nutrient access and reduced competition that permit the unhindered expansion of individual cell lineages, forming genetically segregated sectors11. In contrast, cross-feeding interactions, where one species relies on nutrients or modification of its imminent surroundings provided by another species within the assemblage23 add constraints by the need for close proximity to the interacting partner. The signature of such interactions is seen in the spatial organization of cells within the assemblage24,25,26,27 with the potential of sequential expansion if trophic interactions are unilateral28. Interestingly, these sequential patterns can be interrupted by a second pattern28, where large monoclonal sectors emerge due to rare nucleation events (where monoclonal sectors are seeded due to a combination stochastic but mostly deterministic conditions). These patterns mediate various aspects of community functioning and genetic makeup; the disturbance or absence of spatial structure may adversely impact community ecosystem functions7,29,30. Experimentally resolving the mechanisms that give rise to different community expansion patterns remain a challenge due to difficulties in visualizing and tracking individual cells, and limitations in representing the underlying and highly dynamic nutrient landscape. Turning to mathematical models that simulate both the nutrient conditions and bacterial processes at the relevant scale to individual cells provides an opportunity to unveil mechanisms giving rise to experimentally observed community patterns at the macro scale. We hypothesize that the spatial organization of sessile, cross-feeding bacterial assemblages undergoing range expansion is shaped by highly localized and dynamic differences in cell growth rates that are reinforced by feedbacks, or self-engineered of local nutrient landscape. To systematically and quantitatively evaluate the hypothesis and the mechanisms postulated, we developed an agent-based model that combines Monod type growth kinetics with a simple mechanical shoving algorithm for bacterial growth in homogeneous and structured habitats similar to experimental setups used for independent validation. The detailed description of chemical and metabolite diffusion at high spatial resolution links localized nutrient conditions and spatially variable growth rates as a key driver that promote community pattern formation. Finally, we discuss the influence of obstacles such as found in structured habitats (porous media or rough surfaces) on the spatial self-organization, community proliferation, and genetic segregation. Our modelling framework provides novel mechanistic insights into experimental observations of spatial self-organization during bacterial range expansion, predicting a feedback between the emerging colony pattern and self-engineered nutrient landscape at a resolution currently inaccessible to experimental quantification. These insights are used to visualize the importance of the spatial dimension in shaping the community composition concerning individual “lucky” bacterial lineages and potential ramification for evolutionary mechanisms.


Dynamic nutrient landscapes mediate colony spatial self-organization

We use a synthetic community containing two isogenic mutants of P. stutzeri A150128,31 cross-feeding nitrite in the denitrification pathway (Fig. 1a) to systematically investigate mechanisms, that shape the spatial self-organization of trophically interacting bacterial colonies during range expansion. The inherent toxicity of nitrite at low ambient pH modify the type of trophic interactions from competition (complete reducer growing anaerobically on nitrate, negative bilateral), via weak mutualism (producer and consumer cross-feeding nitrite anaerobically at pH 7.5, positive unilateral) to strong mutualism (producer and consumer cross-feeding nitrite anaerobically at pH 6.5, positive bilateral). Consequently, we observe experimentally two fundamentally different expansion mechanisms depending on the type of trophic interactions. Competition for the same resource fosters segregation and the formation of well-defined sectors of each bacterial strain (Fig. 1b). Similar patterns have been observed frequently in other studies11,28,31. The onset of strong mutualistic interactions promote an increased intermixing of the two strains (Fig. 1c) that we attribute to the need for reducing diffusion distances between interacting partners30,31. Weak mutualistic growth invokes two distinct spatial patterns: a sequential pattern where producer cells dominate the colony periphery28,31, and in certain rare cases where large consumer branches emerge at the colony periphery (Fig. 1d). The dynamics of super-sectors (defined as the rare but large monoclonal sectors observed in weak mutualistic scenarios contributing disproportionally to colony expansion) are difficult to investigate experimentally and require insights into the spatially variable growth rates and shoving mechanisms.

Fig. 1: Spatial patterns emerging from different trophic interactions among members of a synthetic bacterial community grown on agar surfaces.

a The denitrification metabolic pathway of the complete reducer and the producer and consumer used in this study. The complete reducer P. stutzeri A1501 employs the entire denitrification pathway, reducing nitrate (NO3) all the way to dinitrogen gas (N2). Two nitrite cross-feeders derived from the complete reducer were used to form a mutualistic consortium: (i) a producer converts nitrate to nitrite (NO2) but is unable to complete the denitrification pathway due to a lack of nitrite reductase; (ii) a consumer unable to use nitrate directly as an electron acceptor (lacking the enzyme nitrate reductase) and thus depends on the producer supplying nitrite. The toxicity of the intermediate metabolite nitrite promotes a mutualistic relationship where the strength of the interaction is controllable due to the variable toxicity of nitrite depending on local pH (acidity). b Comparison of experimental and simulation data of a competitive scenario represented by two complete reducer P. stutzeri strains. Simultaneous expansion of the two isogenic but fluorescently tagged strains creates visible sectors of strains tagged with the same fluorescence. c Comparison of experimental and simulation data of a mutualistic interaction, where producer is tagged with CFP (blue) and consumer with GFP (green). Due to the higher toxicity of nitrite the community is more intermixed. d Comparison of experimental and simulation data of a weak mutualistic (pH 7.5) scenario where producer is tagged with ecfp (blue) and consumer with egfp (green). The colony follows sequential expansion lead by the producer with visible sectors of consumers emerging.

The mathematical model reveals strong links between the underlying nutrient landscape and localized growth rates that shape the colony patterns (Fig. 2). When observing the nutrient conditions in the proximity of the expanding colony edge (indicated by the red rim in Fig. 2d), both complete reducer strains experience the same nitrate concentrations and hence equal growth rates as they are essentially isogenic strains in the competitive scenario (Fig. 2a). Strong mutualism (nitrite being toxic, pH 6.5) results in a lower but similar growth rate (converging) of the two bacterial strains, hence, smaller colony size for the same incubation time when compared to the competition scenario. A significantly different pattern characterizes the weak mutualistic consortium. After an initial lag phase due to nitrite unavailability, the consumer strain benefits from an overall higher growth rate compared to the producer strain in the weak mutualistic scenario (Fig. 2a). This mechanism is rooted in the underlying nutrient landscape (Fig. 2b, c). At pH 6.5, nitrite toxicity controls the proliferation of the consumer strain and equal production and consumption keep nitrite concentrations low. At pH 7.5, nitrite is nontoxic and begins to accumulate during the early stages of colony growth due to the sequential expansion of the producer followed by the consumer. In some rare cases, consumers are pushed ahead by the proliferating producers (Fig. 2d) and remain in the actively growing colony periphery. Once sufficient nitrite is available, these consumer cells residing at the periphery proliferate disproportionally due to their relative growth rate advantage and create large monoclonal consumer sectors. This process, remaining at the periphery through passive motion until favorable conditions enable emergence of super sectors, is further defined as “nucleation of super-sectors” for simplicity. These differences become apparent when visualizing dynamic growth rates of individual agents during the simulation depending on the location and strain (Fig. 2d). Producer cells remaining at the colony periphery retain high growth rates throughout the simulation slightly declining due to nitrate diffusive limitations. Consumer cells on the other hand have an initial disadvantage owing to the lack of nitrite, which first needs to be provided by the producer cells. Thus, consumer cells are reliant on proliferation and shoving from producer cells to stay at the colony periphery. Once the surrounding producers provide sufficient nitrite, the cells which managed to remain at the colony periphery proliferate into large sectors of kin cells due to a relative growth rate advantage compared to the surrounding producers (no substrate limitation). These observations highlight how stochastic effects (shoving of the consumer cells through producer proliferation) and deterministic processes (higher relative growth rate of the relocated consumer cells resulting in concave sector boundaries) manage to govern the two different observed patterns in weak mutualistic conditions.

Fig. 2: The underlying chemical landscape governs local growth rates of the bacterial colony.

Nutrient concentrations and growth rates within the growth layer for all trophic interactions (red zone in c). a In the competitive scenario, predicted growth rates are equal for the complete reducers having the same kinetic parameters. Weak mutualism is characterized by a relative growth rate advantage due to the ubiquitous nitrite availability. In mutualistic scenario, both strains have a lower but equal growth rate due to nitrite toxicity, emphasizing their mutualistic interaction. Dynamics of nitrate (b) and nitrite (c) for all trophic interactions. Competition results in a slow decline of nitrate with no nitrite produced (complete reducer). Weak mutualistic conditions promote the accumulation of nitrite as there is negligible toxicity in this condition. Strong mutualism results in a rapid decline of nitrate (toxicity acts on the yield), with overall low nitrite levels (removed by consumer cells in close proximity). d Spatial distribution of the two species community in weak mutualistic conditions (top) in relation to the predicted growth rates (bottom) at the end of the simulation time. Following individual cells within the simulation reveals different growth rate histories depending on the strain and location. Growth rates of producer cells are dictated by nitrate availability and proximity to the colony periphery (due to nitrate diffusion). Consumer cells initially cannot grow due to nitrite limitation and subsequently proliferate if remaining sufficiently close to the colony periphery through shoving. Rare nucleation events indicate the creation of large monoclonal sectors that arise due to favorable spatial positioning (initially shoved by the producer cells) and nutrient conditions.

Lineage tracking reveals lucky individuals and spatial genetic bottlenecks

The mechanistic model offers opportunities that are not yet possible experimentally, namely to track linages of bacterial “virtual” cells within the complex and spatially varying community. The assumption is that variations in reproductive success of the ancestral population (inoculated cells) results in some cell lineages (defined as the ancestral inoculated cell and all of its progeny), that contribute disproportionally to the final colony biomass as depicted as pseudo-colors in Fig. 3. For competitive trophic interactions, the model predicts a clear segregation of the two strains into sectors that prominently persist into the colony periphery (as also observed experimentally shown in Fig. 1a and in other studies). An important observation that could not be resolved in the experiment is that a single sector containing the same strain does not consist of a single ancestor (i.e., not originating from the same inoculated cell). Strong mutualism favors intermixing of the two strains with considerably thinner sectors compared to the trophic competition scenario. Sequential expansion as observed under weak mutualistic interactions alters the observed pattern. For the majority of the colony, the producer expands radially (perpendicular to the colony periphery) with no penetration of consumer sectors similar to the pattern observed in the competitive scenario (essentially equal patterns since producers compete for nitrate). Super sectors that penetrate the layer of producers are typically monoclonal, owing to the fact that they typically nucleate from a single cell (ratio of consumer lineages at the periphery to consumer branches is 1.25 ± 0.05). In between consumer branches, an increased rate of coalescence of producer lineages can be observed that arise from spatial bottlenecks imposed by the flanking consumer sectors. The degree to which a community de-mixes during range expansion experiments is commonly quantified by counting the number of transitions between different strain sectors at the colony periphery, and can be tracked dynamically in the simulation (Fig. 3b, legend in Fig. 3c). For competitive trophic interactions, the total visible sectors remain stable throughout the simulation with a slight negative trend due to coalescence events, where individual sectors are pinched and buried behind the colony expansion front. Sequential expansion of two strains promotes rapid demixing for weak mutualistic interactions, with some more branches resurging in the later stages of the simulation.

Fig. 3: Trophic interactions alter the reproductive success of individual cells.

a Reproductive success of individual lineages with associated spatial patterns of demixing depending on trophic interaction. Competition results in well-defined sectors where one sector typically contains multiple ancestral lineages. Strong mutualism favors intermixing of the two strains resulting thin sectors. In case of weak mutualism, the producer strain primarily engages in competitive patterns due to nutrient competition with its kin. Large consumer sectors emerge where individual ancestral lineages become dominant and produce monoclonal sectors. b The number of interspecies boundaries remains stable in the competitive scenario. In weak mutualistic scenario, the number of interspecies boundaries shows a decline due to the loss of most consumer branches. An increase in the number of interspecies boundaries in the strong mutualistic case is attributed to branches bifurcating and thus increased intermixing of the two strains. c The total number of unique lineages residing at the colony periphery shows a steep decrease during early colony development asymptotically reaching steady state once sectors have developed. The decrease follows different patterns depending on trophic interactions mediated by the varying mechanisms of range expansion (sequential vs. simultaneous). Each scenario was replicated six times.

For the strong mutualistic interactions scenario, the tight association between the two strains favors intermixing and thus an overall higher number of individual branches is seen at the end of the simulations. The modelling results follow capabilities of the experimental system, where distinction between sectors can only be made based on fluorescent differentiation. By quantifying the unique lineages that proliferate to the colony periphery, differences in demixing dynamics between the strains become evident. When competing for the same resource, the two strains demix very rapidly, as they are essentially equivalent except for the fluorescent label (Fig. 3c). In the case of strong mutualism, demixing of both strains is slower compared to the competitive case where more individual lineages manage to proliferate at the colony periphery in the case of the consumer strain. Weak mutualism promotes a strong demixing of the consumer strain whereas the producer has a slower demixing with time compared to the competitive scenario, since more space is available initially lacking growth by the consumer until sufficient nitrite has accumulated. Overall, from the inoculated cells residing within the actively growing layer at the colony periphery, approximately 80% of all cell lineages are lost during range expansion which increases to 99% when taking into account all inoculated cells (i.e., cells at the colony center). The loss of lineages during colony expansion underlines the variation in reproductive success of individual lineages, where a fraction of the initial inoculum (0.31% ± 0.02%, 0.32% ± 0.03%, and 4.96% ± 0.06% for the competitive, weak mutualistic, and strong mutualistic scenario, respectively) contributes more than 50% of the final community biomass.

Spatial structure mediates self-organization with genetic consequences

Definitive studies for disentangling the effects of structured environments (porous media or rough surfaces) from those induced by trophic interactions on the resulting spatial organization and genetic lineages are rare. We have used the model to simulate, for identical trophic scenarios (competition, weak mutualism, and strong mutualism) the resulting community patterns expanding in structured environments with varying density of obstacles simulated as solid particles (Fig. 4a–c). An increase in obstacle density results in a higher genetic segregation of the two strains when competing for the same nutrient (Fig. 4a, competition) with fewer individual cell lineages persisting to the colony periphery (Fig. 4d). A similar effect is expected for the producer strain in weak mutualistic conditions, as they are equally dependent on the diffusion of nitrate from the periphery. The increase in physical obstacles has a different effect on the consumer strain branches in the weak mutualistic case (Fig. 4b). Although a similar number of monoclonal consumer branches emerge in the early stages of colony expansion, the obstacles hindered the proliferation of these branches resulting in a limited number persisting to the colony periphery in medium and fine structured habitats (Fig. 4e). Interestingly, more consumer branches persist to the periphery in coarse conditions compared to a homogeneous habitat. Emerging consumer branches are pushed through bottlenecks by surrounding producer cells, which facilitates their persistence to the periphery. In contrast to the medium and fine structured habitats, these branches do not encounter many additional obstacles that may inhibit their proliferation. Strong mutualistic conditions favor a higher degree of intermixing resulting in shorter average diffusion lengths (Fig. 4c). Including obstacles in the simulation results in decreased intermixing of the two strains and thus longer average diffusion lengths expressed in an overall lower total biomass created during colony growth (Fig. 4f).

Fig. 4: Simulated two-species bacterial colony expansion into domains with different spatial solid structures—impacts on lineage proliferation with potential ecological and evolutionary consequences.

Visualization of the influence of a structured environment on the emerging colony pattern for competing (a), weak mutualism (b), and strong mutualism (c) in relation to the structure density. d When competing, the addition of structures reduces the number of cell lineages proliferating to the periphery due to trapping of cell lineages in front of the obstacle. This leads to greater genetic segregation of the community and fewer lineages persisting to the assemblage periphery. e Weak mutualistic conditions result in a similar picture concerning producers. Consumer branches that nucleate in front of an obstacle are limited in their persistence due to spatial constrains and the total number of proliferating branches decrease with increasing obstacle density changing the ecological functioning of the assemblage. Interestingly, the introduction of coarse obstacles to a homogeneous habitat increases the number of consumer branches (although statistically not significant, p-value of 0.12, two-sample t-test). f In mutualistic conditions, the increased segregation of the two strains is detrimental to the function of the whole community due to the increased diffusion distance between the strains resulting in an overall lower expansion rate of the community. Quantification of the unique peripheral lineages, peripheral consumer branches, and biomass is summarized in SI Table 1. Six replicates were simulated for scenarios void of obstacles. For each scenario containing obstacles, ten replicates were simulated.


It has been frequently documented that changes in trophic interactions invoke fundamentally different spatial self-organization and expansion mechanisms such as simultaneous expansion when competing for the same resource11,28,31, simultaneous expansion at higher intermixing ratios during strong mutualistic growth30,31,32 or sequential expansion for cross-feeding an intermediate metabolite with positive unilateral of the interacting species28. In the latter case, two significantly different patterns are observed within the same colony: (i) sequential expansion where the producer strain advances first and the consumer strain follows and (ii) localized super-sectors of the consumer strain having a higher growth rate compared to the surrounding producer strain28,31. Important questions concerning these super-sectors are the mechanisms that promote the emergence of the super sectors and their persistence at the colony periphery. In order for super sectors to emerge, two conditions are required: an initial phase where consumers manage to stay at the periphery despite a growth rate disadvantage and a subsequent phase, where consumers have a growth rate advantage indicated by the curved sector boundaries. In the simulations, growing producer cells initially shove consumers located at the colony periphery until sufficient nitrite is produced for them to proliferate.

An in-depth experimental evaluation of the importance of initial spatial positioning, and the role of cell shoving is complex due to massive amount of replicates and inability to remove cell shoving in a living community. Alternatively, we have removed the shoving component in the mathematical model (i.e., allowing only peripheral cells contribution to colony expansion through placement of their progeny on unoccupied grid nodes). The result was an overall lower expansion of the colonies (SI Fig. 1a–c) with conspicuous omission of super sectors in the weak mutualistic scenario (SI Fig. 1b). Additionally, we could easily control the initial positioning of consumers and producers in the mathematical model. Encasing the colony with consumer cells resulted in myriads of consumer super sectors (SI Fig. 1d), whereas encasing the inoculated colony with producer cells suppressed the emergence of any consumer super sectors as they are buried behind the advancing producer front. These additional simulations highlight the importance of initial spatial positioning and cell shoving for the seeding of the observed consumer super sectors, in case of the weak mutualistic scenario.

The mechanism enabling the consumer individuals to proliferate disproportionate compared to the producer at the colony periphery is embedded within the underlying nutrient landscape, where localized relative growth rate differences between the two strains emerge dynamically (Fig. 2d). In contrast to the producer, the consumer strain is not dependent on diffusion of peripheral nitrate and has a ubiquitous supply of nitrite provided by the more abundant producer, resulting in a higher growth rate relative to the producer in the later stages of colony expansion (Fig. 2b, c). In comparison to other processes that result in spatially self-organized patterns such as the classical Turing pattern processes33 or phase separation34, the spatial organization in our model is governed by localized growth conditions, self-engineered metabolic landscapes and favorable initial spatial positioning that differ fundamentally from the system properties in both the above-mentioned theories. The shape of the emerging super sector has previously been linked to the relative growth rate advantages35. Similar observations have been made in studies focusing on the mechanical forces shaping the spatial patterns of mutant strains with relative growth rate differences during range expansion17,18. In both cases, cells having a growth rate disadvantage managed to stay at the colony periphery through mechanical interactions, and shoving of the surrounding faster growing cells. Although the resulting colony pattern in our system is similar to the above-mentioned studies, where growth rate differences are imposed via mutations and are thus fixed in time, the mechanism is fundamentally different. In our simulations however, the emerging spatial organization of the synthetic community is a feedback of self-engineered nutrient landscapes that drive localized growth conditions. This highlights the interplay of biotic and abiotic factors during community assembly of sessile bacterial assemblages, and the importance of localized growth rates as a key driver for emerging spatial self-organization.

Genetic segregation of fluorescently labelled strains in experiments suggests a strong reduction in genetic diversity compared to the ancestral population11. Limited by the availability of differentiable fluorescent proteins, experimental observations are restricted to a coarse resolution and are not capable of resolving individual lineages, although efforts have been made to include multiple fluorescent proteins13, high temporal resolution imaging36, and also three dimensional tracking37. An individual-based model on the other hand is capable to resolve the segregation dynamics based on individual inoculated cells, and enabled us to quantify the number of individual cell lineages persisting at the expanding colony edge depending on trophic interaction. Interestingly, comparison of demixing dynamics show a similar trend for strong mutualism and competition when looking at individual lineages compared to the strain-based differentiation, i.e., a higher intermixing in the case of the mutualistic scenario versus competitive (Fig. 3b, c). In the weak mutualistic case, the producer benefits from the reduced competition for space (since the consumer initially does not grow due to the lack of nitrite) resulting in more individual cell lineages proliferating and persisting at the colony periphery. Only once the consumer super-sectors begin to emerge do they begin to pose a barrier for the producer cells resulting in coalescence events and an overall reduction of observed producer cell lineages at the colony periphery. For the case of consumer cells, weak mutualistic growth results in a few “lucky cells” that are able to proliferate and contribute disproportionally to the colony expansion. These cell lineages, despite being dependent on another strain, profit from the weak mutualistic growth, which highlights the somewhat counterintuitive situation of having a higher reproductive success compared to any other scenario despite an initial growth rate disadvantage.

Bacterial assemblages rarely grow on homogeneous surfaces and the spatial context has been shown to strongly influence the community stability and function with respect to trophic interactions38. The influence of single objects and rough agar on the proliferation of cell lineages has been observed both experimentally and in silico39,40,41. Specifically, a recent study investigated the growth and spatial self-organization of trophically interacting synthetic communities during range expansion with the inclusion of a spatially structured habitat42. Other recent studies include the interrelation of structure and flow environment on biofilm growth43, the influence of hydration conditions7 and boundary deformities42 on the spatial organization of trophically interacting communities7 and the influence of heterogeneous environments on population genetics41. Simplified, cell lineages directly in front of the obstacles are outgrown by lineages close to the obstacle boundary, posing spatial genetic bottlenecks19,39,40. When growing in a habitat populated by numerous solid obstacles, this effect is amplified and results in a more pronounced genetic segregation compared to the homogeneous environment void of obstacles with an overall reduction of individual cell lineages residing at the colony periphery. Because natural habitats are rarely homogeneous (as growth on agar pates and in some of the simulations), we explored scenarios with stochastic variations in the size and spacing of obstacles (solid grains or pillars) that showed a similar trend when compared to the simulation results with regular spaced grids (SI Fig. 2, SI Table 1).

Within the simulations, cells were treated as isogenic without any genetic variation or potential for mutations. In natural bacterial assemblages, a higher number of individual cell lineages containing genetic variation and potential mutations at the expanding edge increases the opportunity for natural selection to shape the final community structure44. It has been shown previously that allele surfing promotes adaptation of bacterial colonies using a mutation with tunable selective advantage36. Again, one of the main differences between this and our system is the fact that the relative growth rate advantage is a dynamic emergent property of the underlying nutrient landscape. Thus, the observed mechanisms of localized growth rates shaping the dynamics of individual cell lineages has the potential of modulating evolutionary processes by determining the standing genetic variation of the expanding edge in natural bacterial assemblages. This in turn accelerates (increased beneficial mutations at the periphery) or decelerates (burying beneficial mutations behind the expanding front) the pace of evolution in bacterial assemblages undergoing range expansion36. It is generally thought that a balance between genetic drift and natural selection shapes the population genetics of range expanding communities. We here showed in addition how trophic interactions and nutrient availability underlying bacterial communities can shape the proliferation of individual cells through localized growth rate advantages, and thus alter evolutionary mechanisms acting within the growth layer. Spatially structured habitats mediate the reproductive success of individual lineages and highlight the importance of chance relative to natural selection for trophically interacting bacterial communities. Our simulations and experimental validation emphasize the importance of growth rate differences as a key driver in pattern formation and final genetic population diversity, and the importance of microbes as “environmental engineers” playing a crucial role in not only shaping their imminent surroundings but also having far-reaching consequences for community structure and local ecosystem functioning.


Experimental observations using a synthetic bacterial community

A previously established synthetic cross-feeding bacterial ecosystem composed of two isogenic mutant strains of the bacterium Pseudomonas stutzeri A150128,45 was used as a model community (Fig. 1). Briefly, the producer strain is able to reduce nitrate to nitrite but not further to nitrous oxide. The consumer on the other hand can only reduce nitrite to nitrous oxide but is unable to use nitrate. When grown together with nitrate as the growth-limiting resource, the two strains engage in a nitrite cross-feeding interaction. Nitrite is toxic at pH 6.5 but not at pH 7.546,47,48,49, thus the cross-feeding interaction can be fine-tuned between weak mutualism and stronger mutualism by adjusting the pH of the growth medium or agar plate. When growing aerobically, the manipulated range of pH does not have any experimentally observable effect on liquid growth capabilities45. The two strains also contain an IPTG-inducible green or cyan fluorescent protein-encoding gene28, which enables us to distinguish and quantify the abundance of each strain when grown together28,31. Two complete reducers differentiated by the same IPTG-inducible fluorescent proteins are used to create a scenario where both strains compete for nitrate (competition)50.

Experimental range expansion

The range expansion experiments were performed as described in Goldschmidt28. We prepared overnight cultures of the complete reducers alone and the cross-feeding isogenic mutants alone in lysogeny broth (LB) medium for a period of 12 h in a shaking incubator at 37 °C at 220 rpm. When the cultures reached stationary phase, the optical density at 600 nm (OD600) was adjusted to one. In order to adjust the OD, the cultures were centrifuged at 3615 × g for 8 min, the supernatants were discarded, and the remaining cells were suspended in 1000 µl of 0.9% (w/v) NaCl solution. We then transferred the cultures into a glove box (Coy Laboratory Products, Grass Lake, MI) containing a nitrogen (N2):hydrogen (H2) (97:3) anaerobic atmosphere. Two strains (two complete reducers or producer and consumer) were mixed at a ratio of 1:1 and 1 µl were then deposited onto the center of anaerobic LB agar plate amended with 1 mM of sodium nitrate (NaNO3) and adjusted to pH 7.5 (weak mutualistic conditions) or 6.5 (strong mutualistic conditions) with 0.5 M NaOH or 30% v/v HCl. Plates were incubated in the anaerobic glove box for a period of 2 weeks at room temperature. The colonies were subsequently imaged using a Leica TCS SP5 II confocal microscope (Etzlar, Germany). The colonies were exposed to aerobic conditions for 1 h preceding image acquisition to allow for maturation of the fluorescent proteins.

Agent-based mathematical model

The mathematical model combines numerical pseudo two-dimensional nutrient diffusion with an on-grid individual-based representation of bacterial cells following local growth conditions determined using Monod-type kinetics7,51,52. A circular domain of 5 mm radius composed of a hexagonal lattice with side length of 20 microns is used as a backbone for diffusion calculation based on one-dimensional Fickian diffusion between nodes whilst respecting mass balance (consumption and production of the respective nutrients) at each node (Eq. 1):

$$\begin{array}{*{20}{c}} {\frac{{\partial C_{{\mathrm{NO}}_{3}}}}{{\partial t}} = D\frac{{\partial ^2C_{{\mathrm{NO}}_{3}}}}{{\partial x^2}} - \frac{{\mu _{{\mathrm{prod}}}}}{{Y_{{\mathrm{NO}}_{3}}}}\frac{{\partial m_{{\mathrm{prod}}}}}{{\partial t}}} \\ {\frac{{\partial C_{{\mathrm{NO}}_{2}}}}{{\partial t}} = D\frac{{\partial ^2C_{{\mathrm{NO}}_{2}}}}{{\partial x^2}} - \frac{{\mu _{{\mathrm{cons}}}}}{{Y_{{\mathrm{NO}}_{2}}}}\frac{{\partial m_{{\mathrm{cons}}}}}{{\partial t}} + \frac{{\mu _P}}{{Y_{{\mathrm{NO}}_{3}}}}\frac{{\partial m_{{\mathrm{prod}}}}}{{\partial t}}} \end{array},$$

where CNO3 and CNO2 is the concentration of nitrate and nitrite [mol/m3], t is time [s], D the diffusion coefficient [m2/s], x the spatial coordinate along the bond [m], μprod and μcons the growth rate of producer and consumers [1/s], YNO3 and YNO2 the biomass yield on nitrate and nitrite [kgDW/mol] and mprod and mcons the biomass of producer and consumers [kg]. Details of how the individual components are calculated is shown in Eqs. (27) with all parameters given in Table 1. Only nitrate and nitrite are included in the simulation since other nutrients are provided in nonlimiting concentrations. A constant peripheral source for nitrate is included (setting the concentration at the boundary nodes to 1 mM before the numerical diffusion step), whereas nitrite is produced locally solely by bacterial metabolism. Due to the size of each hexagon, bacterial cells are essentially represented as super agents53, and each grid node is inhabited by a single cell (i.e., strains are mutually exclusive).

Table 1 List of modelling parameters and references.

Bacterial cells are inoculated at the center (inoculation radius of 2 mm) where each node is attributed randomly with a producer or consumer strain. A random inoculation mass for each superagent is chosen between 10 and 100% of the mass at division.

Bacterial cells consume nutrients depending on the trophic interaction. In the competitive scenario, both strains only consume nitrate where the growth rate for a super-agent i (i.e., node i of the grid) is calculated using Eq. 2:

$$\mu _{{\mathrm{cd}},i} = \mu _{\max } \ast \frac{{C_{{\mathrm{NO}}_3,i}}}{{C_{{\mathrm{NO}}_3,i} + K_{{\mathrm{NO}}_3}}},$$

where μcd,i is the local growth rate of the complete reducer [1/s] at node i, μmax the maximum growth rate [1/s], KNO3 the Monod half-saturation coefficient for nitrate [mM] and CNO3,cd the nitrate concentration [mM] at node i. When cross feeding on nitrite (weak mutualism, i.e., no nitrite toxicity), the growth rates of the producer and consumer are described by Eqs. (3) and (4), respectively:

$$\mu _{{\mathrm{prod,}}i}\,=\,\mu _{{{\max}} } \ast \frac{{C_{{\mathrm{NO}}_3,{{i}}}}}{{C_{{\mathrm{NO}}_3,{{i}}} + K_{{\mathrm{NO}}_3}}},$$
$$\mu _{{\mathrm{cons,}}i}\,=\,\mu _{{{\max}} } \ast \frac{{C_{{\mathrm{NO}}_2,{{i}}}}}{{C_{{\mathrm{NO}}_2,{{i}}} + K_{{\mathrm{NO}}_2}}},$$

where μprod,i is the local growth rate of producer cell [1/s] at node i, μcons,i is the local growth rate of consumer cell [1/s] at node i, KNO2 the Monod half-saturation coefficient for nitrite [mM], and CNO2,i the nitrite concentration [mM] at node i. Biomass dynamics follow a simple exponential model as described by Eq. (5):

$$m_{{{t + 1,i}}} = m_{{{t,i}}} + \mu _{{i}} \ast m_{{{t,i}}} \ast {\Delta}t$$

where mt+1,i and mt,i is the biomass [kg] in time step t and t + 1 at node i, respectively, and ∆t the numerical time step [s]. The total nutrient consumed is related to the gain in biomass at node i following a biomass yield coefficient described by Eq. (6)

$$\vartheta _{{{n,i}}} = \frac{{\mu _i \ast m_{t,i}}}{{Y_i}},$$

where ϑn,i is the consumption rate of nutrient n at node i [mol/s] and Yi the biomass yield coefficient [kgDW/mol]. In the case of nitrate consumption by the producer, an equivalent amount of nitrite is produced following stoichiometry. Nitrite toxicity has been shown to affect the growth yield54. Thus, for the mutualistic conditions, the biomass yield coefficient for both strains is calculated using Eq. (7):

$$Y_{{i}} = \left\{ {\begin{array}{*{20}{c}} {\left( {Y_{\max } - Y_{\min }} \right) \ast \frac{{K_{{\mathrm{inh}}}}}{{K_{{\mathrm{inh}}} + C_{{\mathrm{NO}}_2,{{i}}}}} + Y_{\min },\,{\mathrm{pH}} = 6.5} \\ {Y_{\max },\,{\mathrm{pH}} = 7.5} \end{array}} \right.$$

where Ymax is the maximum biomass yield [kgDW/mol], Ymin the minimum biomass yield [kgDW/mol], and Kinh the nitrite inhibition coefficient [mM].

Colony expansion in the mathematical model is a combination of cell division and a simple on-grid cell shoving algorithm. Upon reaching intrinsic critical mass for division, a bacterial cell divides into two where one daughter cell occupies the current location and the second either occupies an adjacent cell (if the location is unoccupied or cell shoving is permitted), or is added to the current location in a layer above (pseudo three-dimensional colony growth). From the location of a dividing cell, the shortest path distance to the colony periphery is calculated. If the distance is sufficiently small (<100 µ, five grid cells) all cells along the shortest path are (mathematically) shoved towards the colony periphery, where the current peripheral cell is assigned a new node at random from any of the unoccupied neighboring nodes. The physical obstacles (in the structured scenarios) are treated as solid and impenetrable domain boundaries. The structured habitats were simulated by adding solid obstacles of defined dimensions (100 µ diameter) spaced regularly within the domain (500, 400, and 300 µ for the coarse, medium, and fine structured scenarios). Stochastic obstacle simulations in SI Fig. 2 contained the medium and fine spacing, with obstacle diameters taken from a normal distribution with mean 100 µ, and variance 20 µ. The total simulated time is 72 h using a 60 s time step.

Statistics and reproducibility

Following the procedure outlined in the “Methods” section, distinct colony patterns emerged reproducibly for the different trophic interactions. Simulation results were compared to multiple experimental replicates (a single experimental replicate is provided in this study). For the mathematical simulations, six replicates of the nonstructured scenario and ten for all structured scenarios were generated per trophic interaction. Here, a replicate is defined as simulations containing the same initial and boundary conditions, where stochasticity is included through random position during inoculation and during the simulation via the shoving algorithm. When statistically comparing different simulation results (e.g., biomass, number of branches etc.), two-sample t-tests were used.

Data availability

The experimental data (microscopy images) that support the findings of this study are available within the manuscript and supporting information.

Code availability

The mathematical code that support the findings of this study is available in the ETH Research Collection with the identifier 10.3929/ethz-b-00043269055.


  1. 1.

    Hall-Stoodley, L., Costerton, J. W. & Stoodley, P. Bacterial biofilms: from the natural environment to infectious diseases. Nat. Rev. Microbiol. 2, 95–108 (2004).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  2. 2.

    Kolter, R. & Greenberg, E. P. Microbial sciences: the superficial life of microbes. Nature 441, 300–302 (2006).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  3. 3.

    Monds, R. D. & O’Toole, G. A. The developmental model of microbial biofilms: ten years of a paradigm up for review. Trends Microbiol. 17, 73–87 (2009).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  4. 4.

    Nadell, C. D., Xavier, J. B. & Foster, K. R. The sociobiology of biofilms. FEMS Microbiol. Rev. 33, 206–224 (2009).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  5. 5.

    Flemming, H. C. & Wuertz, S. Bacteria and archaea on Earth and their abundance in biofilms. Nat. Rev. Microbiol. 17, 247–260 (2019).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  6. 6.

    Stewart, P. S. Diffusion in biofilms. J. Bacteriol. 185, 1485–1491 (2003).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  7. 7.

    Borer, B., Tecon, R. & Or, D. Spatial organization of bacterial populations in response to oxygen and carbon counter-gradients in pore networks. Nat. Commun. 9, 1–11 (2018).

    CAS  Article  Google Scholar 

  8. 8.

    Testa, S. et al. Spatial structure affects phage efficacy in infecting dual-strain biofilms of Pseudomonas aeruginosa. Commun. Biol. 2, 1–12 (2019).

    CAS  Article  Google Scholar 

  9. 9.

    Justice, S. S., Hunstad, D. A., Cegelski, L. & Hultgren, S. J. Morphological plasticity as a bacterial survival strategy. Nat. Rev. Microbiol. 6, 162–168 (2008).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  10. 10.

    Hallatschek, O. & Nelson, D. R. Population genetics and range expansions. Phys. Today 62, 42 (2009).

    CAS  Article  Google Scholar 

  11. 11.

    Hallatschek, O., Hersen, P., Ramanathan, S. & Nelson, D. R. Genetic drift at expanding frontiers promotes gene segregation. Proc. Natl Acad. Sci. 104, 19926–19930 (2007).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  12. 12.

    Weber, M. F., Poxleitner, G., Hebisch, E., Frey, E. & Opitz, M. Chemical warfare and survival strategies in bacterial range expansions. J. R. Soc. Interface 11, 20140172 (2014).

  13. 13.

    Weinstein, B. T., Lavrentovich, M. O., Möbius, W., Murray, A. W. & Nelson, D. R. Genetic drift and selection in many-allele range expansions. PLoS Comput. Biol. 13, e1005866 (2017).

  14. 14.

    Van Gestel, J., Weissing, F. J., Kuipers, O. P. & Kovács, Á. T. Density of founder cells affects spatial pattern formation and cooperation in Bacillus subtilis biofilms. ISME J. 8, 2069–2079 (2014).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  15. 15.

    Mitri, S., Clarke, E. & Foster, K. R. Resource limitation drives spatial organization in microbial groups. ISME J. 10, 1–12 (2016).

    Article  CAS  Google Scholar 

  16. 16.

    Müller, M. J. I., Neugeboren, B. I., Nelson, D. R. & Murray, A. W. Genetic drift opposes mutualism during Spatial population expansion. Proc. Natl Acad. Sci. USA 111, 1037–1042 (2014).

    PubMed  Article  CAS  PubMed Central  Google Scholar 

  17. 17.

    Giometto, A., Nelson, D. R. & Murray, A. W. Physical interactions reduce the power of natural selection in growing yeast colonies. Proc. Natl Acad. Sci. 115, 11448–11453 (2018).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  18. 18.

    Kayser, J., Schreck, C. F., Gralka, M., Fusco, D. & Hallatschek, O. Collective motion conceals fitness differences in crowded cellular populations. Nat. Ecol. Evol. 3, 125–134 (2019).

    Article  Google Scholar 

  19. 19.

    Travis, J. M. J. et al. Deleterious mutations can surf to high densities on the wave front of an expanding population. Mol. Biol. Evol. 24, 2334–2343 (2007).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  20. 20.

    Odling-Smee, F. J., Laland, K. N. & Feldman, M. W. Niche construction. Am. Nat. 147, 641 (1996).

    Article  Google Scholar 

  21. 21.

    Cole, J. A., Kohler, L., Hedhli, J. & Luthey-Schulten, Z. Spatially-resolved metabolic cooperativity within dense bacterial colonies. BMC Syst. Biol. 9, 1–17 (2015).

    CAS  Article  Google Scholar 

  22. 22.

    Dal Co, A., Ackermann, M. & van Vliet, S. Metabolic activity affects the response of single cells to a nutrient switch in structured populations. J. R. Soc. Interface 16, 20190182 (2019).

  23. 23.

    Estrela, S. et al. Environmentally mediated social dilemmas. Trends Ecol. Evol. 34, 6–18 (2019).

    PubMed  Article  PubMed Central  Google Scholar 

  24. 24.

    Rohani, P., Lewis, T. J., Grünbaum, D. & Ruxton, G. D. Spatial self-organization in ecology: Pretty patterns or robust reality? Trends Ecol. Evol. 12, 70–74 (1997).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  25. 25.

    Camazine, S. et al. Self-Organization in Biological Systems. (Princeton University Press, Princeton, 2003).

  26. 26.

    Lion, S. & Baalen, M. Van Self-structuring in spatial evolutionary ecology. Ecol. Lett. 11, 277–295 (2008).

    PubMed  Article  PubMed Central  Google Scholar 

  27. 27.

    Dong, X. & Fisher, S. G. Ecosystem spatial self-organization: Free order for nothing? Ecol. Complex. 38, 24–30 (2019).

    Article  Google Scholar 

  28. 28.

    Goldschmidt, F., Regoes, R. R. & Johnson, D. R. Successive range expansion promotes diversity and accelerates evolution in spatially structured microbial populations. ISME J. 11, 2112–2123 (2017).

    PubMed  PubMed Central  Article  Google Scholar 

  29. 29.

    Haagensen, J. A. J., Hansen, S. K., Christensen, B. B., Pamp, S. J. & Molin, S. Development of spatial distribution patterns by biofilm cells. Appl. Environ. Microbiol. 81, 6120–6128 (2015).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  30. 30.

    Tecon, R. & Or, D. Cooperation in carbon source degradation shapes spatial self-organization of microbial consortia on hydrated surfaces. Sci. Rep. 7, 43726 (2017).

    PubMed  PubMed Central  Article  Google Scholar 

  31. 31.

    Goldschmidt, F., Regoes, R. R. & Johnson, D. R. Metabolite toxicity slows local diversity loss during expansion of a microbial cross-feeding community. ISME J. 12, 136–144 (2018).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  32. 32.

    Momeni, B., Brileya, K. A., Fields, M. W. & Shou, W. Strong inter-population cooperation leads to partner intermixing in microbial communities. Elife 2013, 1–23 (2013).

    Google Scholar 

  33. 33.

    Karig, D. et al. Stochastic Turing patterns in a synthetic bacterial population. Proc. Natl Acad. Sci. USA 115, 6572–6577 (2018).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  34. 34.

    Liu, Q. X. et al. Phase separation explains a new class of selforganized spatial patterns in ecological systems. Proc. Natl Acad. Sci. USA 110, 11905–11910 (2013).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  35. 35.

    Farrell, F. D., Gralka, M., Hallatschek, O. & Waclaw, B. Mechanical interactions in bacterial colonies and the surfing probability of beneficial mutations. J. R. Soc. Interface 14, 20170073 (2017).

  36. 36.

    Gralka, M. et al. Allele surfing promotes microbial adaptation from standing variation. Ecol. Lett. 19, 889–898 (2016).

    PubMed  PubMed Central  Article  Google Scholar 

  37. 37.

    Díaz-Pascual, F. et al. Breakdown of Vibrio cholerae biofilm architecture induced by antibiotics disrupts community barrier function. Nat. Microbiol. 4, 2136–2145 (2019).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  38. 38.

    Lowery, N. V. & Ursell, T. Structured environments fundamentally alter dynamics and stability of ecological communities. Proc. Natl Acad. Sci. USA 16, 379–388 (2019).

    Article  CAS  Google Scholar 

  39. 39.

    Möbius, W., Murray, A. W. & Nelson, D. R. How obstacles perturb population fronts and alter their genetic structure. PLoS Comput. Biol. 11, e1004615 (2015).

  40. 40.

    Beller, D. A. et al. Evolution of populations expanding on curved surfaces(a). EPL 123, 58005 (2018).

  41. 41.

    Gralka, M. & Hallatschek, O. Environmental heterogeneity can tip the population genetics of range expansions. Elife 8, e44359 (2019).

  42. 42.

    Ciccarese, D., Zuidema, A., Merlo, V. & Johnson, D. R. Interaction-dependent effects of surface structure on microbial spatial self-organization. Philos. Trans. R. Soc. Lond. B Biol. Sci. 375, 20190246 (2020).

  43. 43.

    Nadell, C. D., Ricaurte, D., Yan, J., Drescher, K. & Bassler, B. L. Flow environment and matrix structure interact to determine spatial competition in Pseudomonas aeruginosa biofilms. Elife 6, e21855 (2017).

  44. 44.

    Kayser, J., Schreck, C. F., Yu, Q., Gralka, M. & Hallatschek, O. Emergence of evolutionary driving forces in pattern-forming microbial populations. Philos. Trans. R. Soc. B Biol. Sci. 373, 20170106 (2018).

  45. 45.

    Lilja, E. E. & Johnson, D. R. Segregating metabolic processes into different microbial cells accelerates the consumption of inhibitory substrates. ISME J. 10, 1568–1578 (2016).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  46. 46.

    Almeida, J. S., Reis, M. A. M. & Carrondo, M. J. T. Competition between nitrate and nitrite reduction in denitrification by Pseudomonas fluorescens. Biotechnol. Bioeng. 46, 476–484 (1995).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  47. 47.

    Sijbesma, W. F. H., Almeida, J. S., Reis, M. A. M. & Santos, H. Uncoupling effect of nitrite during denitrification by Pseudomonas fluorescens: an in vivo 31 P-NMR study. Biotechnol. Bioeng. 52, 176–182 (1996).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  48. 48.

    Baumann, B., Van Der Meer, J. R., Snozzi, M. & Zehnder, A. J. B. Inhibition of denitrification activity but not of mRNA induction in Paracoccus dentrificans by nitrite at a suboptimal pH. Int. J. Gen. Mol. Microbiol. 72, 183–189 (1997).

    CAS  Google Scholar 

  49. 49.

    Zhou, Y., Oehmen, A., Lim, M., Vadivelu, V. & Ng, W. J. The role of nitrite and free nitrous acid (FNA) in wastewater treatment plants. Water Res. 45, 4672–4682 (2011).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  50. 50.

    Lilja, E. E. & Johnson, D. R. Metabolite toxicity determines the pace of molecular evolution within microbial populations. BMC Evol. Biol. 17, 1–12 (2017).

    Article  CAS  Google Scholar 

  51. 51.

    Ebrahimi, A. & Or, D. Hydration and diffusion processes shape microbial community organization and function in model soil aggregates. Water Resour. Res. 51, 9804–9827 (2015).

    Article  Google Scholar 

  52. 52.

    Kim, M. & Or, D. Individual-based model of microbial life on hydrated rough soil surfaces. PLoS ONE 11, e0147394 (2016).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  53. 53.

    Scheffer, M., Baveco, J. M., Deangelis, D. L., Rose, K. A. & Vannes, E. H. Super-individuals a simple solution for modeling large populations on an individual basis. Ecol. Model. 80, 161–170 (1995).

    Article  Google Scholar 

  54. 54.

    Thatipamala, R., Rohani, S. & Hill, G. A. Effects of high product and substrate inhibitions on the kinetics and biomass and product yields during ethanol batch fermentation. Biotechnol. Bioeng. 40, 289–297 (1992).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  55. 55.

    Borer, B., Ciccarese, D., Johnson, D. R. & Or, D. Spatial organization in microbial range expansion emerges from trophic dependencies and successful lineages: source code. (2020).

  56. 56.

    Kreft, J. U., Picioreanu, C., Wimpenny, J. W. T. & Van Loosdrecht, M. C. M. Individual-based modelling of biofilms. Microbiology 147, 2897–2912 (2001).

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  57. 57.

    Kornaros, M. & Lyberatos, G. Kinetics of aerobic growth of a denitrifying bacterium, Pseudomonas denitrificans, in the presence of nitrates and/or nitrites. Water Res. 31, 479–488 (1997).

    CAS  Article  Google Scholar 

  58. 58.

    Calderer, M., Jubany, I., Pérez, R., Martí, V. & de Pablo, J. Modelling enhanced groundwater denitrification in batch micrococosm tests. Chem. Eng. J. 165, 2–9 (2010).

    CAS  Article  Google Scholar 

  59. 59.

    Kornaros, M. & Lyberatos, G. Kinetic modelling of Pseudomonas dentrificans growth and denitrification under aerobic, anoxic and transient operating conditions. Water Res. 32, 1912–1922 (1998).

    CAS  Article  Google Scholar 

  60. 60.

    Kornaros, M., Zafiri, C. & Lyberatos, G. Kinetics of denitrification by Pseudomonas denitrificans under growth conditions limited by carbon and/or nitrate or nitrite. Water Environ. Res. 68, 934–945 (1996).

    CAS  Article  Google Scholar 

Download references


Financial support for this work came from an Advanced Grant to D.O. by the European Research Council (ERC-3200499-‘SoilLife’) and from the RTD project ‘MicroscapesX’ and grants from the Swiss National Science Foundation (grant numbers 31003A_149304 and 31003A_176101) awarded to D.J.

Author information




B.B., D.C, D.J., and D.O. conceived the study and wrote the manuscript. D.C. performed the experiments including visualization. B.B. wrote the mathematical model, created simulation scenarios and analyzed the data.

Corresponding author

Correspondence to Benedict Borer.

Ethics declarations

Competing interests

The authors declare no competing interests.

Additional information

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Borer, B., Ciccarese, D., Johnson, D. et al. Spatial organization in microbial range expansion emerges from trophic dependencies and successful lineages. Commun Biol 3, 685 (2020).

Download citation


By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.


Quick links

Nature Briefing

Sign up for the Nature Briefing newsletter — what matters in science, free to your inbox daily.

Get the most important science stories of the day, free in your inbox. Sign up for Nature Briefing