Compatible solutes including simple sugars, heterosides, and amino acids are accumulated intracellularly to protect cells from heating, freezing, desiccation, and oxidative stress (Welsh, 2000). Compatible solutes balance osmotic pressure, help maintain cell turgor pressure, can be used as an energy source, and protect cellular structures against changes in water availability. Studies have been conducted on many Pseudomonas strains demonstrating their ability to synthesize compatible solutes to overcome different types of stress (Kurz et al., 2010; Sandhya et al., 2010).

One of the most well studied compatible solutes is the disaccharide trehalose. Trehalose is a stable, colorless non-reducing disaccharide that is used to stabilize products in cosmetics, food, and pharmaceuticals (Schiraldi et al., 2002). There are two proposed mechanisms to explain the desiccation protection properties of trehalose. The first mechanism is that trehalose provides protection by encasing biomolecules in a glass sugar matrix which halts molecular mobility and degradation (Jain and Roy, 2009). The second is the water replacement hypothesis which explains that trehalose protects the native protein conformation during drying by replacing the hydrogen bonds formed between water and the protein with hydrogen bonds formed between the trehalose hydroxyl group and the protein (Mensink et al., 2017).

The ability to accumulate and synthesize trehalose has been identified in Pseudomonas and is accomplished through the action of trehalose-P-synthase and trehalose-P-phosphatase enzymes encoded by otsA and otsB homologs (Lee et al., 2005; Park et al., 2007). The accumulation of trehalose by Pseudomonas sp. BCNU 106 was determined by measuring the total intracellular trehalose content, trehalase activity, and mRNA levels of the trehalose-biosynthetic genes (Park et al., 2007). Pseudomonas strains have been screened for the presence of trehalose synthase to produce trehalose from maltose. Trehalose synthase has been discovered in P. stutzeri and P. putida strains, and this enzyme has been cloned and expressed in Escherichia coli (E. coli) for scaled-up production (Lee et al., 2005; Wang et al., 2014). Trehalose has been demonstrated to protect Pseudomonas strains from toxic organic solvents, desiccation, salt stress, and other environmental stressors (Mikkat et al., 2000; Park et al., 2007; Freeman et al., 2010).

Glutamate and the derivatives of this amino acid play essential roles in nitrogen metabolism and stress tolerance. Alpha ketoglutarate, an intermediate of the TCA Cycle, is utilized by P. fluorescens for detoxification of reactive oxygen species (Mailloux et al., 2009). Alpha ketoglutarate eliminates reactive oxygen species by reacting with hydrogen peroxide to form succinate, water, and carbon dioxide (Liu et al., 2018). During oxidative stress alpha ketoglutarate dehydrogenase is downregulated, leaving alpha ketoglutarate molecules to scavenge reactive oxygen species and protect the cell (Mailloux et al., 2009).

Glutamine synthetase was downregulated in P. syringae strains in response to osmotic shock (Freeman et al., 2013). Under these conditions, glutamine synthetase would no longer catalyze a conversion of glutamate to glutamine resulting in an accumulation of glutamate. Freeman and associates theorize glutamate may function as a counterion to positively charged potassium ions before transitioning to glutamine synthesis. This hypothesis for glutamates function in osmotic stress has also been demonstrated in studies conducted on the model organism E. coli (Cagliero and Jin, 2013). Exogenous potassium ions are brought into the cell to maintain the osmotic or turgor pressure after osmotic stress. To compensate for the net charge increase from the intake of potassium ions, glutamate is accumulated or synthesized so the net charge of the cytoplasm is preserved.

Pseudomonas strains have developed numerous mechanisms to survive exposure to stress in the natural environment. The knowledge gained from studying bacterial mechanisms of survival can be applied to industrial processing. Protectants can be externally applied to beneficial strains to increase viability especially during the formulation process. The formulation process is necessary to enhance the storage capability, transportability, and ease of application in the field. Typically, bacterial strains are grown and harvested from broth, protectants are externally added to the harvested cells, then the cells are dried using methods such as spray drying or freeze drying (Berninger et al., 2018). Protectants can also be added to the medium during growth to be taken up and accumulated in the cell for a protective effect.

There are a number of protectants available including sugars (e.g., sucrose, trehalose, maltose, and lactose), polyols (e.g., mannitol, sorbitol, and glycerol), and amino acids (e.g., L-leucine, Glycine, and L-Proline). Research has been conducted to identify optimal protectants for the formulation of Pseudomonas biological control agents. One study was carried out to identify optimal osmoprotectants for three P. fluorescens strains capable of reducing Fusarium dry rot of potatoes (Schisler et al., 2016). The osmoprotectants glucose, fructose, trehalose, raffinose, and stachyose were applied to the strains before air drying. Fructose and trehalose were shown to be the most effective osmoprotectants overall though osmoprotectant influence on cell survival varied between strains. Lactose proved to be an optimal lyoprotectant for freeze drying and cold storage of a P. fluorescens strain utilized for the control of fire blight disease (Cabrefiga et al., 2014), whereas maltodextrin improved the viability after fluidized bed drying of a P. protegens strain capable of controlling bacterial wilt of tomatoes (Wang et al., 2020b). Elucidation of bacterial mechanisms of stress survival has informed the application of protectants during industrial fermentation and formulation processes and is an area of continued research interest for further refining and improving effectual protectant supplementation.

Biofilms are composed of a complex consortium of microorganisms that are adhered to a surface and are encased in an extracellular matrix. The extracellular matrix is composed of extracellular polymeric substances (EPSs) secreted by the cells living in the biofilm such as polysaccharides, proteins, glycoproteins, glycolipids, and extracellular DNA (Flemming et al., 2007; Lopez et al., 2010). The EPS primarily functions to maintain biofilm integrity and to provide protection against desiccation and other stresses. Biofilm formation supports the transition of formerly vegetative cells to non-dividing, antibiotic resistant persister cells, which further enhances their resistance to biotic and abiotic stresses (Lopez et al., 2010).

Polysaccharides are a predominant component of biofilms and help facilitate aggregation, adherence, and surface tolerance (Mann and Wozniak, 2012). Alginate is an exopolysaccharide that plays a major role in Pseudomonas biofilm formation by affecting the biofilm structure and stress resistance (Hentzer et al., 2001). Alginate protects cells from water limitation by controlling biofilm architecture and hydration (Gulez et al., 2014). Alginate absorbs and retains water allowing cells to stay hydrated long enough to metabolically adjust to desiccation conditions. Alginate production during water limiting stress in P. putida strain mt-2 resulted in taller biofilms covering less surface area with a thicker EPS layer compared to the algD mutant strain (Chang et al., 2007). Alginate deficiency was shown to decrease stress tolerance in biocontrol and plant growth promoting strains of P. putida and P. fluorescens (Svenningsen et al., 2018; Marshall et al., 2019).

Several more polysaccharides are capable of supporting Pseudomonas sp. biofilm integrity including levan and the polysaccharide synthesis locus (psl) dependent polysaccharide. Levan has been hypothesized as a source of nutrient stores to protect cells within the biofilm from starvation (Mann and Wozniak, 2012). Studies of P. syringae biofilm formation demonstrated an increase in the levan forming enzyme, levansucrase, during planktonic exponential growth and storage of levan in cell-depleted voids within microcolonies (Laue et al., 2006). The psl-dependent polysaccharide consists of a repeating pentasaccharide containing D-mannose, D-glucose, and L-rhamnose (Byrd et al., 2009). The deletion of psl genes has been demonstrated to dramatically decrease biofilm formation in P. aeruginosa (Ma et al., 2012). In addition, the comparison of alginate or Psl producing strains revealed that overproduction of alginate leads to mucoid biofilms, which occupy more space, while Psl-dependent biofilms are densely packed.

Detrimental biofilms have become a major problem in healthcare, food, and agricultural industries. The resilience of biofilms to stress has led to significant issues with contaminants persisting through sterilization procedures. P. aeruginosa has caused persistent infections in immunocompromised patients through biofilm formation on medical equipment (Hadi et al., 2009). P. syringae has been isolated from irrigation water and epilithic biofilms (Morris et al., 2008). Biofilms can become the source of infection in agricultural fields by contaminating irrigation systems with plant pathogens (Raudales et al., 2014). In addition, biofilms can build up in pipes, tubing, and tanks causing persistent contamination during the fermentation and processing of microbial products (Rich et al., 2015). Many strategies including chelating agents, peptide antibiotics, lantibiotics and synthetic chemical compounds have been developed to control biofilms in industrial processing (Roy et al., 2018).

Biological control agents can be encapsulated by surrounding the bacteria with coats of material such as polymers to create small capsules (Huq et al., 2013). Encapsulation can be used to protect biological control agents from stress and slowly release the bacteria over longer periods of time. Alginate is a common material for encapsulation because it is biodegradable, non-toxic, and easy to handle (Power et al., 2011). Several P. fluorescens strains have been encapsulated with alginate formulations to study the impact on storage survival and pathogen control (Pour et al., 2019; Kadmiri et al., 2020). P. fluorescens strains VUPF5 and T17-4 were encapsulated with an alginate-gelatin formulation which improved shelf life and control of dry rot induced by Fusarium solani under greenhouse conditions (Pour et al., 2019). The microbial fertilizer P. fluorescens Ms-01 was encapsulated with halloysite and alginate or montmorillonite and alginate formulations (Kadmiri et al., 2020). Both formulations were able to preserve bacterial survival after 3 months storage at room temperature or 4°C. Encapsulation of microorganisms in a semipermeable membrane separates and protects the cells from the surrounding environment (Pour et al., 2019). This method protects biological control agents from abiotic stresses allowing proliferation in the environment and effective deployment against plant pathogens.

Bacteria must make rapid responses to the changing environment by forming and replacing cellular proteins. Molecular chaperones are proteins that play a critical role in this process by assisting with the correct folding and assembly or disassembly of other proteins (Lawless and Hubbard, 2014). Chaperones remain important under non-stressed conditions as self-assembly of some proteins occur at slower rates and can lead to misfolding or aggregation of partially folded intermediates (Alix, 2006). A rapid increase in chaperone synthesis occurs under heat and other stress conditions to control the aggregation of denatured proteins.

GroEL and DnaK are two well characterized chaperone systems conserved throughout many bacteria (Singh and Gupta, 2009). The heat shock protein system GroEL/GroES consists of the 60 kDa chaperonin GroEL that forms two stacked rings in a barrel-like structure and a 10 kDa cofactor GroES that forms a single ring structure (Alix, 2006). An unfolded protein binds to the hydrophobic amino acid residues on the interior rim of the GroEL ring opening (Georgescauld et al., 2014). ATP binds to GroEL inducing a conformational change allowing GroES to attach and close off GroEL. This formation results in an enclosed cage with a hydrophilic interior leading the unfolded protein to release from the rim and refold. ATP hydrolysis and protein binding to the opposite ring causes GroES and the protein to release.

Research on heat shock response in Pseudomonas has revealed a GroEL/GroES system similar to the system found in the model organism E. coli (Ito et al., 2014). The GroES/GroEL system was found in P. aeruginosa PAO1 through S1 nuclease mapping and northern hybridization with a two-fold upregulation under heat shock (Fujita et al., 1998). The groES and groEL region is conserved amongst Pseudomonas species. In fact, the 536 bp region of the groE gene was used to develop a diagnostic PCR assay for detection of P. aeruginosa, P. putida, P. fluorescens, and P. stutzeri (Clarke et al., 2003).

The DnaK, DnaJ, and GrpE chaperone system prevents proteins that are damaged or stuck in an intermediate folded state from aggregating. The system consists of the chaperone DnaK, the co-chaperone DnaJ, and the nucleotide exchange factor GrpE. DnaK is a 70 kDa chaperone with an ATP-binding N-terminal, a substrate binding domain, and a peptide binding C-terminal domain (Mayer et al., 2000). The hydrophobic amino acid residue of misfolded proteins will bind to the substrate binding domain of DnaK. DnaJ will promote hydrolysis of ATP to ADP at the N-terminal ATPase domain (Alderson et al., 2016). When ADP is bound, the C-terminal domain locks down on the protein by closing off the substrate-binding site. DnaJ dissociates and the complex will continue to hold the protein. GrpE binds leading to a conformational change that releases ADP and shifts DnaK to an open conformation.

Several studies have been conducted to better understand the role of DnaK in the Pseudomonas heat shock response. Transcriptome analysis was performed on P. aeruginosa PAO1 grown at human body temperature (37°C) and an elevated temperature (46°C) (Chan et al., 2016). RNA sequencing revealed 133 genes were differentially expressed including the upregulation of dnaK, dnaJ, and groEL at 46°C compared to human body temperature. The heat shock response of P. putida KT2442 was elucidated by constructing and testing null mutants of molecular chaperone genes (Ito et al., 2014). The P. putida KT2442 dnaJ mutant was temperature-sensitive and formed more protein aggregates in response to heat stress compared to the wild type.

Proteases are crucial for rapid responses to environmental changes when damaged proteins cannot be salvaged by chaperones or other heat shock proteins. Proteases are enzymes that catalyze the breakdown of proteins into amino acids or smaller polypeptides by cleaving peptide bonds. They contribute to the heat shock response by removing misfolded or damaged proteins and recovering the amino acids (Meyer and Baker, 2011). Proteases will also degrade functional proteins such as sigma factors, metabolic enzymes and structural proteins that are no longer needed as cells adapt to changes (Kirstein et al., 2009; Bittner et al., 2016). The Clp protease family is a highly conserved system that is vital for stress survival in many bacteria, including Pseudomonas species.

Clp complexes contain chaperones and proteases that belong to the heat shock protein family HSP100 and the ATPases Associated with diverse cellular Activities (AAA+) protein superfamily. The AAA+ superfamily has a highly conserved AAA+ module consisting of 250 amino acids, and they typically have motifs involved in ATP binding and hydrolysis (Ogura and Wilkinson, 2001). ATP-dependent Clp protease (ClpP) consists of a ClpP serine peptidase subunit and a AAA+ ATPase subunit such as ClpA, ClpC, or ClpX (Richter et al., 2010). ClpP forms a barrel-like structure with two stacked heptameric rings of the ClpP serine peptidase subunit and is enclosed by one or two hexameric rings of the AAA + ATPase subunit. The Clp ATPase subunit uses ATP hydrolysis to unfold protein substrates then directs them through a central pore to the proteolytic chamber of ClpP for degradation (Snider et al., 2008).

Clp Peptidase has been found to control diverse aspects of cellular physiology in Pseudomonas species. The proteolysis activity of ClpP helps regulate the stress response sigma factor RpoS (σ38) and other transcriptional regulators influencing many factors including motility, surface attachment, and antimicrobial activity (Bruijn and Raaijmakers, 2009). P. aeruginosa was found to have a second ClpP isomer which impacts stationary-phase cells, microcolony organization and biofilm formation (Hall et al., 2017). ClpP, clpX, and clpP2 null mutants of P. aeruginosa PAO581 were created to study the regulation of exopolysaccharide alginate overproduction and the conversion to a mucoid phenotype which are markers for the onset of chronic lung infection in cystic fibrosis patients (Qiu et al., 2008). All null mutants demonstrated a decrease in transcriptional activity of the extracytoplasmic function sigma factor AlgU which is responsible for alginate overproduction. The clpP and clpX null mutants were unable to maintain the mucoid phenotype.

Chaperones and Proteases such as DnaK and Clp control the regulation of cyclic lipopeptides in many Pseudomonas species. Cyclic lipopeptides have a role in biofilm formation, surface motility, and antimicrobial activity (Dubern et al., 2005). Putisolvin and massetolide have activity against oomycete plant pathogens by causing lysis of zoospores (Raaijmakers et al., 2010). The DnaK complex is hypothesized to regulate putisolvin biosynthesis by controlling activity of other regulators or assisting with the assembly of putisolvin peptide synthetases. ClpP regulates massetolide biosynthesis by degradation of putative transcriptional repressors of massetolide biosynthesis genes (Bruijn and Raaijmakers, 2009). A range of growth temperatures (32, 28, 21, 16, and 11°C) were tested on a P. Putida strain and three dnaK, dnaJ, and grpE mutants to determine the effect on putisolvin production (Dubern et al., 2005). It was shown that putisolvin production decreased at high growth temperatures, but putisolvin production increased at low temperatures. DnaK and DnaJ are required to produce putisolvins at low temperatures. These studies indicate that growth temperature can influence DnaK and DnaJ regulation of putisolvin synthesis, and growth at low temperatures may enhance putisolvin production. Chaperones and proteases are key components to survival and efficacy for many Pseudomonas species. Understanding regulatory effects of these proteins is crucial to the development of Pseudomonas strains as biocontrol products.

Adverse environmental conditions such as elevated temperatures can damage proteins requiring molecular chaperones or proteases to help repair cells. Thermosensors are RNA, DNA, or protein molecules that react to changes in environmental conditions and regulate gene expression of the heat shock response and other stress responses. Temperature shifts cause thermosensors to change their secondary structure, and this change typically either exposes or blocks nucleic acid regions influencing expression of a gene. DNA topology can act as a stress sensor because transcription efficiency is sensitive to changes in DNA supercoiling (Klinkert and Narberhaus, 2009). RNA thermosensors are translational control elements that are mostly located in the 5′ untranslated region (UTR) of messenger RNA encoding heat shock proteins (Narberhaus, 2010). There are a diverse set of protein thermosensors including transcriptional repressors, sensor kinases, chaperones, and proteases (Collin and Schuch(eds), 2009). The diversity is due to the sensitivity of tertiary and quaternary protein structures to temperature stress (Klinkert and Narberhaus, 2009).

Repression of heat shock gene expression (ROSE) elements are RNA thermosensors located in the 5’ UTR of some heat shock protein mRNA (Nocker et al., 2001). ROSE elements structures consist of two to four stem loops and they are characterized by a conserved G residue that pairs with the Shine Dalgarno sequence (AGGA) (Klinkert and Narberhaus, 2009). Under normal conditions, the conserved G residue opposite the Shine Dalgarno sequence closes the loop by a weak GG base pair preventing gene expression. The weak GG base pair breaks under temperature stress allowing the ribosome binding site to be accessed for translation.

Structural and functional analysis has uncovered the ROSE elements’ role in heat shock and virulence regulation for Pseudomonas species. P. putida and P. aeruginosa contain a simpler ROSE element with only two hairpins compared to previously discovered Rhizobium sp. ROSE structures with three to four hairpin structures (Nocker et al., 2001; Krajewski et al., 2013). The ROSE element precedes an ibpA gene which encodes the small heat shock protein IbpA (inclusion body associated protein A). High sequence conservation of ibpA untranslated regions suggests ROSE thermosensors could be common for IbpA regulation in Pseudomonas species. ROSE elements have also been studied for the temperature induced regulation of rhamnolipid production in Pseudomonas species. Bioremediation strains of Pseudomonas produce rhamnolipids which facilitate the uptake and degradation of hydrocarbons such as crude oil in polluted environments (Chrzanowski et al., 2012). P. aeruginosa is one of the most competent rhamnolipid producers and safe methods to produce rhamnolipids are being explored including strain engineering to diminish pathogenicity (Chong and Li, 2017). P. putida KT2440 rhamnolipid production increased by more than 60% when growth temperature was increased from 30 to 37°C (Noll et al., 2019). These studies demonstrate the potential to design a process for rhamnolipid production linked to temperature and ROSE regulation.

Sigma factors are essential for regulation of both essential genes and conditional responses such as heat or cold shock. A sigma factor is a protein required for transcription initiation that allows RNA polymerase to bind to specific gene promoters. Primary sigma factor (σ70) is named for its 70 kDa molecular weight, and it is responsible for regulation of essential genes during exponential growth. Sigma factor 70 binds to RNA polymerase allowing promoter recognition at —10 and —35 nucleotides upstream of the start site (Potvin et al., 2008). Alternative sigma factors are needed for transcription of genes linked to environmental or physiological changes. In response to stress RNA polymerases are redirected by alternative sigma factors to activate transcription of genes to help the cell respond to new conditions.

Genome analysis of P. aeruginosa PAO1 and P. syringae pv. syringae B728a revealed the presence of 24 and 15 putative sigma factors, respectively, including primary sigma factor (σ70), heat shock sigma factor (σ32), stationary phase sigma factor (σ38), and nitrogen-limitation sigma factor (σ54) (Potvin et al., 2008; Thakur et al., 2013). The majority were classified as extracytoplasmic function (ECF) sigma factors which are involved in the regulation of a diverse set of functions including iron starvation, cell envelope stress, solvent tolerance, and oxidative stress (Otero-Asman et al., 2019). Stationary phase sigma factor RpoS (σ38) is a master stress response regulator active during stationary phase to protect against heat shock, starvation, and osmotic shock (Schuster et al., 2004). The heat shock sigma factor RpoH (σ32) was upregulated as temperature increased from 30 to 42°C in P. aeruginosa (Nakahigashi et al., 1998). RpoH regulates heat shock genes responsible for the expression of chaperones and proteases such as GroEL, GroES, DnaK, DnaJ, GrpE, and ClpP (Aramaki et al., 2001; Potvin et al., 2008). Sigma Factor AlgU (σ22) mutant strains of Pseudomonas fluorescens CHA0 were studied to determine the impact of AlgU on environmental stress survival (Schnider-Keel et al., 2001). Schnider-Keel et al. (2001) found that AlgU is critical for survival against desiccation and hyperosmolarity in soil environments. Alternative sigma factors are critical to survival against major industrial and environmental stresses.

Cold shock proteins (csp) and cold acclimation proteins (cap) are two strategies Pseudomonas strains utilize to adapt to cold environments. Genes encoding cold shock proteins are expressed immediately after cold shock while genes encoding cold acclimation proteins are expressed during prolonged exposure to low temperatures (Trevors et al., 2012). Cold shock proteins are transcriptional anti-terminators or translational enhancers that destabilize RNA secondary structure at low temperatures (Nakaminami et al., 2006). This destabilization of RNA secondary structure prevents premature transcription termination during cold shock. Cold acclimation proteins have been found to have a high level of amino acid sequence identity to members of the CspA family of E. coli and the homologous proteins of other microorganisms (Berger et al., 1997). CapA contained highly conserved ribonucleoprotein (RNP1 and RNP2) involved with binding to single stranded DNA and RNA, suggesting similar functionality to Csp proteins.

The expression level of a cold shock protein from P. fluorescens MTCC 103 (MW 14 kd) and a cold resistant protein (MW 35kd) from the P. fluorescens mutant CRPF8 were studied over a range of temperatures from 37°C down to 4°C (Khan et al., 2003). Expression of the cold shock protein and the cold resistant protein increased in response to decreased temperature with the rate of induction of protein synthesis reaching its maximum at 10°C. Eighteen Pseudomonas strains isolated from Antarctica were analyzed for the presence of cold shock proteins and cold accumulation proteins (Panicker et al., 2010). CapB was present in all Antarctic Pseudomonas isolates, but CspA was absent. The survival of these isolates in the perennially cold Antarctic environment could be attributed to the continuous expression of CapB and its regulatory role in transcription and translation of essential genes.

Antifreeze proteins also called ice structuring proteins are ice-binding proteins produced by certain organisms to enhance survival in freezing temperatures. Antifreeze proteins inhibit the spread of ice by lowering the freezing point and preventing ice recrystallization (Venketesh and Dayananda, 2008). Antifreeze activity is theorized to occur by an adsorption inhibition mechanism where antifreeze proteins bind to ice crystals and curved ice structures form between the antifreeze proteins. Due to the Kelvin effect, the curved surface is energetically less favorable than flat surfaces which prevents additional water molecules from joining the ice formation (Wang et al., 2017). Ice recrystallization, where ice crystals gradually grow larger in size at the expense of smaller ice crystals, is a lethal stress for cells in frozen conditions. Antifreeze proteins can prevent recrystallization by inhibiting water molecules from leaving ice crystals or by acting as a surfactant to reduce surface tension.

The freezing resistance of antifreeze proteins was discovered in several cold dwelling Pseudomonas species including strains of P. ficuserectae, P. fluorescens, and P. putida (Kawahara et al., 2004; Singh et al., 2014; Cid et al., 2016). Freeze sensitive mutants and a freeze resistant wild type strain of the plant growth-promoting rhizobacterium P. putida GR12-2 were tested for the ability to secrete antifreeze proteins (Kawahara et al., 2001). The freeze sensitive mutants secreted a much lower concentration of antifreeze protein compared to the wild type. Freeze resistance could be partially restored by adding purified antifreeze proteins to the freeze sensitive mutant’s cell suspension. The antifreeze gene afpA from P. putida GR12-2 was cloned into E. coli yielding a 72 kDa protein that exhibited low levels of antifreeze and ice nucleation activities compared to the native protein (Muryoi et al., 2004). The recombinant protein may not have been properly post translationally modified with previous work indicating the carbohydrate lipoglycoprotein was required for ice nucleation activity. These studies demonstrate the potential of accumulated antifreeze proteins to inhibit ice formation in both freeze resistant and freeze sensitive strains.

Altering membrane composition is a critical strategy to combat the rigidity of the cell membrane during cold shock. Membrane fluidity is maintained by increasing the ratio of unsaturated fatty acids to saturated fatty acids or by altering the levels of anteiso branched chain fatty acids in membrane phospholipids (Shivaji and Prakash, 2010). Rigidity of the membrane signals the adjustment to membrane lipid composition through biosynthetic pathways including FabAB and Des mediated pathways. The cis configuration of unsaturated fatty acids has double bonds which produce a bend in the fatty acid chain (Heipieper et al., 2003). These bends create more space between the unsaturated fatty acid chains producing a more flexible and fluid membrane during cold stress.

The synthesis of unsaturated fatty acids by fatty acid desaturase enzymes is essential for the survival of Pseudomonas during cold stress. The cold tolerant strains Pseudomonas sp. AMS8 and Pseudomonas sp. A3 were found to produce large amounts of monounsaturated fatty acids at low temperatures (Garba et al., 2016, 2018). Δ9- fatty acid desaturase genes were isolated from each of the strains and were subsequently cloned and successfully expressed in E. coli. In both studies the recombinant E. coli had a functional putative Δ9-fatty acid desaturase capable of increasing the total amount of cellular unsaturated fatty acids. Functional genomics was used to study the cold stress response in the bacterial model organism P. putida KT2440 (Frank et al., 2011). Transcriptome sequencing and proteome peptide profiling of KT2440 revealed that the degradation pathway of valine to branched-chain fatty acids (bkd operon) was upregulated during growth at low temperatures. These studies illustrate the importance of homeoviscous adaptation to support membrane fluidity during cold stress.

Viable but non-culturable (VBNC) cells have low metabolic activity and intact membranes, but they are unable to replicate until they enter a more hospitable environment (Ayrapetyan et al., 2018). Pseudomonas strains can enter this state as a response to unfavorable environmental conditions such as nutrient limitation, temperature extremes, and desiccation (Lowder et al., 2000; Arana et al., 2010; Pazos-Rojas et al., 2019). Resuscitation methods that allow VBNC cells to repair and transition into a culturable state can vary greatly depending on the type of microorganism and environmental conditions (Bédard et al., 2014). The plant growth-promoting rhizobacterium P. putida KT2440 was found to return to a cultivable state after interaction with maize root exudates or a 48 h rehydration in water (Pazos-Rojas et al., 2019). The persistence of VBNC Pseudomonas in the natural environment was demonstrated with the biocontrol strain P. protegens CHA0 which survived in an uncovered field plot as a combination of dormant and VBNC cells for 72 days (Troxler et al., 2012).

Studies were conducted by Pazos-Rojas et al. (2019) to determine the survival of P. putida KT2440 exposed to desiccation stress. P. putida KT2440 was subjected to 18 days of desiccation then rehydrated with either maize root exudates for a short time or water for 48 h (Pazos-Rojas et al., 2019). Live/dead staining showed that bacterial counts for desiccated and rehydrated cells were just as high as the counts for the bacteria that did not get exposed to stress. Cells exposed to desiccation stress that were neither rehydrated nor protected with trehalose stained red indicating death or a compromised membrane. The presence of VBNC cells after desiccation exposure was tested again with a GFP-tagged P. putida strain which exhibited active GFP expression and housekeeping gene expression was confirmed with RT-PCR. A cytokine secreted by Micrococcus luteus called resuscitation-promoting factor (Rpf) has been discovered which enables the resuscitation of VBNC cells in a wide range of Gram negative and Gram positive bacteria (Su et al., 2013). There is limited information on potential homologous genes in Pseudomonas, but tests could be conducted to determine if adding Rpf to VBNC Pseudomonas cells improves resuscitation.

Biological control agents have a viability standard which is listed on the product label. The company manufacturing the product determines the standard based on product efficacy and typically guarantees a minimum colony-forming unit (CFU) per gram (Cabrefiga et al., 2014; Anderson et al., 2018). The stress of manufacturing live microbial products can lead a fraction of the population to enter a VBNC state (Davis, 2014). VBNC cells can return to a culturable state in more hospitable environmental conditions or by resuscitating microbes through a rehydration process. A large population of VBNC cells which are more difficult to enumerate using traditional plating methods can complicate the process of ensuring the product meets the viability requirements on the label. Two methods to identify culturable and VBNC cells are live/dead staining with microscopic enumeration or detecting housekeeping gene expression by reverse transcription polymerase chain reaction (Li et al., 2014). Understanding the requirements for different metabolic states and improving enumeration techniques are both essential for enabling more accurate viability standards.

Polyphosphate is a polymer containing a few to several hundred phosphate residues linked by high energy phosphoanhydride bonds (Brown et al., 2004). Many bacteria can intracellularly synthesize and degrade polyphosphate with polyphosphate kinases and exopolyphosphatase. Microorganisms accumulate polyphosphate to store energy, and this energy is released by ATP hydrolysis. Polyphosphate is also involved in stress responses including regulation of the stringent response, induction of the stress response sigma factor, and biofilm formation (Nikel et al., 2013; Gray and Jakob, 2014).

The role of polyphosphate was examined with Pseudomonas sp. B4 and P. fluorescens Pf0-1 polyphosphate kinase deficient mutants. Comparative proteomics on the Pseudomonas sp. B4 mutant revealed energy metabolism and nucleoside triphosphate formation were negatively impacted leading to an increase in energy generating metabolic pathways including oxidative phosphorylation and the tricarboxylic acid cycle (Varela et al., 2010). The P. fluorescens Pf0-1 mutant was 10-fold less competitive compared to the wild type strain in sterile soil low in inorganic phosphate, and it had an increased sensitivity to elevated temperatures in sterile soil (Silby et al., 2009). These studies demonstrate the importance of polyphosphate in energy storage and stress response for Pseudomonas species.

Stringent response is a bacterial survival strategy using tRNAs as a sensor to overcome different stressors including nutrient starvation, iron limitation, and heat shock (Vinella et al., 2005; Pletzer et al., 2016). Gene expression switches from growth promotion to survival during stationary phase when nutrients are scarce. The lack of available amino acids leads to an accumulation of ribosomal bound uncharged tRNAs. Binding of uncharged tRNA to the ribosome causes ribosome stalling which triggers RelA synthetase to convert Guanosine-5(’-triphosphate (GTP) into the alarmone guanosine tetraphosphate (ppGpp) (Traxler et al., 2008). SpoT also regulates the stringent response by modifying ppGpp concentration through hydrolysis of ppGpp to guanosine diphosphate (GDP) and pyrophosphate (Boes et al., 2008). ppGpp binds RNA polymerase which halts so that the synthesis of translation machinery (such as ribosomal proteins, rRNA, and tRNA) is decreased, whereas transcription of genes involved in nutrient acquisition, amino acid biosynthesis and stress survival is increased (Wu et al., 2020).

Stringent response is a major factor in stress survival and virulence in both medically and biotechnologically relevant Pseudomonas strains. P. aeruginosa and P. putida stringent response mutants (ΔrelA ΔspoT) were created to test the influence of the stringent response on antioxidant defenses, antibiotic tolerance, biofilm formation, and quorum-sensing (Khakimova et al., 2013; Schafhauser et al., 2014). Studies involving a P. aeruginosa mutant revealed that stringent response regulates catalase activity and hydrogen peroxide tolerance during both planktonic and biofilm growth (Khakimova et al., 2013). Another study on a P. aeruginosa stringent response mutant showed that (p)ppGpp significantly modulates the quorum-sensing hierarchy of a family of molecules controlling antibacterial and virulence functions (Schafhauser et al., 2014). A P. putida stringent response mutant was defective in biofilm dispersal indicating that the stringent response plays a role in relaying the nutrient stress signal to the biofilm dispersal machinery (Díaz-Salazar et al., 2017).

Stringent response has been found to influence the production of secondary metabolites in agriculturally relevant Pseudomonas strains. Pseudomonas species produce antifungal compounds such as pyrrolnitrin and phenazine that inhibit fungal plant pathogens by suppressing mycelial growth (Huang et al., 2018). Stringent response mutants of the biological control agents Pseudomonas sp. strain DF41 and Pseudomonas chlororaphis PA23 were created to stop the production of (p)ppGpp (Manuel et al., 2011; Manuel et al., 2012). The P. chlororaphis PA23 relA mutant had elevated pyrrolnitrin production while phenazine (PHZ) levels remained unchanged. Both P. chlororaphis PA23 and Pseudomonas sp. strain DF41 relA mutants exhibited increased antifungal activity against the pathogen Sclerotinia sclerotiorum (Lib.) de Bary. Expression of secondary metabolites involved in antifungal activity are energetically costly and are reduced during the stringent response when nutrients are scarce (Manuel et al., 2012).

Exposure to sublethal stress is a strategy that has been used to induce the stress response and improve survival during formulation. Pseudomonas biocontrol agents have undergone hyperosmotic adaptation to improve formulation viability and efficacy against pathogens (Cabrefiga et al., 2014; Wang et al., 2020b). Comparative transcriptomic analysis was conducted comparing P. protegens SN15-2 grown under hyperosmotic conditions or normal osmotic conditions then shocked with lethal temperatures (Wang et al., 2020a). The strains were exposed to cold or heat shock from a range of –15°C to 58°C. Exposure to the hyperosmotic environment increased the cytoplasmic concentration of potassium ions, altered the composition of the cell envelope, and increased trehalose and proline synthesis. The accumulation of potassium ions could be a strategy to maintain the osmotic or turgor pressure after osmotic shock (Cagliero and Jin, 2013). Osmotic stress damaged the cell envelope due to salt-induced dehydration leading to an increase in glycerophospholipid metabolism to maintain membrane integrity (Wang et al., 2020a, b). Triggering the stress response with osmotic stress prepared P. protegens SN15-2 for exposure to other stresses such as lethal temperatures.

This strategy of preparing cells with a sublethal shock translates to industrial formulation stress. Stress adaptation by exposure to osmotic shock has been conducted on P. fluorescens EPS62e and P. protegens SN15-2 with improved viability after spray drying and fluidized-bed drying, respectively (Cabrefiga et al., 2014; Wang et al., 2020b). Intentionally triggering the stress response or targeting expression of specific survival mechanisms could enhance survival and colonization in the environment leading to better product performance. As described earlier in this review, Manuel et al. (2012) found that induction of stringent response can decrease the expression of some secondary metabolites involved in antifungal activity. When attempting this method, there needs to be an understanding of what mechanisms of survival are induced and if this will lead to a decrease in the production of the antifungal compound of interest.