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Review

Methods of Identifying Gordonia Strains in Clinical Samples

by
Ekaterina Frantsuzova
1,
Alexander Bogun
1,2,
Anna Vetrova
1 and
Yanina Delegan
1,*
1
Institute of Biochemistry and Physiology of Microorganisms, Federal Research Center “Pushchino Scientific Center for Biological Research of Russian Academy of Sciences” (FRC PSCBR RAS), 142290 Pushchino, Moscow Region, Russia
2
State Research Center for Applied Microbiology and Biotechnology, 142279 Obolensk, Moscow Region, Russia
*
Author to whom correspondence should be addressed.
Pathogens 2022, 11(12), 1496; https://doi.org/10.3390/pathogens11121496
Submission received: 1 November 2022 / Revised: 4 December 2022 / Accepted: 6 December 2022 / Published: 8 December 2022
Versions Notes

Abstract

:
Gordonia spp. are members of the family Gordoniacea in the suborder Corynebacteriales; their habitat, in most cases, is soil. Many representatives of this genus are human or veterinary pathogens. The main cause of the lack of a standardized approach to dealing with infections caused by Gordonia is their erroneous identification and little information regarding their susceptibility to antimicrobial drugs. This review presents the most common methods for identifying Gordonia strains, including modern approaches for identifying a species. The main prospects and future directions of this field of knowledge are briefly presented.

1. Introduction

Gordonia spp. are members of the phylum Actinomycetota, class Actinobacteria, order Actinomycetales, suborder Corynebacterineae, and the family Gordoniacea [1]. Their habitat, in most cases, is soil. Modern literature concerning Gordonia can be divided into several areas, the main of which is the study of the ability of these organisms to utilize various pollutants. Gordonia strains capable of utilizing alkanes [2,3,4], polycyclic aromatic compounds (PAHs) [5,6,7], thiophenes [8,9,10,11], and rubber [12,13,14] are known. The metabolic flexibility of Gordonia strains puts them on par with Rhodococcus, known degraders of various pollutants.
According to the List of Prokaryotic Names with Standing in Nomenclature (https://lpsn.dsmz.de/ (accessed on 30 October 2022)), the Gordonia genus currently consists of 53 species, four of which (“Gordonia australis”, “Gordonia jacobaea”, “Gordonia pseudoamarae”, “Gordonia terrea”) are not validated, and Gordonia nitida is a later heterotypic synonym of Gordonia alkanivorans [15]. In addition to the ability to degrade organic pollutants, Gordonia strains are interesting as producers of secondary metabolites, biosurfactants (glycolipids [16,17], lipopeptides [18], and lipoglycoproteins [19,20]), and carotenoids [21,22,23,24].
Although most Gordonia species have been isolated from environmental samples, several members of this genus were initially isolated from clinical specimens and are considered opportunistic human pathogens [25] (Table 1).
Other cases of Gordonia pathogenesis have been detected in species, representatives of which are usual environmental strains capable of degrading various pollutants (Table 2).
Thus, representatives of 18 of the 53 Gordonia species may be pathogenic to humans and animals.
In most cited sources, patients were immunosuppressed, and infections by Gordonia species occurred secondarily [25]. However, there are also cases of people not immunocompromised and having no medical device but being affected by Gordonia [49,50]. Cases of Gordonia lesions are most common in adults, but several examples of infections in children are known. For example, in 1994, a 3-year-old boy presented with a brain abscess caused by G. terrae [51]. Blaschke et al. [52] observed inflammatory processes in children; in all cases, the cause was Gordonia strains, e.g., G. terrae, G. otitidis, and G. bronchialis. In the work of Ramanan et al. [53], one of the cases of infection was also in a child; the strain was identified as Gordonia sp.
The Gordonia strains themselves are not the cause of death. However, in most cases, pathogenic strains infect immunocompromised patients, and death most often occurs from a general worsening of the state of health [54,55].
There are also cases when, as a result of antibiotic therapy, the symptoms of the Gordonia lesion disappeared, but after a while, the patient died from progressive disease [40,56,57,58].
Bloodstream infections caused by Gordonia strains are often detected in patients with medical devices (Hickman central venous catheter (CVC), etc.) [54,59]. Extracellular biosurfactants with a polysaccharide structure help them form biofilms [60]. This allows Gordonia strains to adhere to rubber material in catheters [61]. Werno et al. [62] revealed that biofilms also reduce the penetration of antibiotics and contribute to the emergence of drug resistance in Gordonia strains.
Gordonia strains can cause infections in other animals besides humans. In veterinary medicine, they are known as the cause of mastitis, mainly in cows [38].
The present review aims to summarize the main modern methods of identifying Gordonia strains and provides a brief summary of therapy approaches.

2. Biochemical Approaches

The representatives of the Gordonia genus are slow-growing, and biochemical identification of these strains is time-consuming, labor-intensive, and usually inconclusive [63]. The biochemical parameters for the discrimination of Gordonia strains from other actinomycetes include the following: acid-fast staining, evaluation of aerial hyphae and the sensitivity to lysozyme, the production of nitrate reductase, and urea hydrolysis [1,64].

2.1. Medium Engineering

For Gordonia cultivation, standard microbiological media, including solid Löwenstein–Jensen, Columbia agar with 5% sheep erythrocytes, Sabouraud agar, chocolate agar, and liquid Schaedler medium, are often used [65,66,67]. Cultivation is usually performed on agarized media, as this allows the evaluation of the appearance and purity of the isolates.
Gordonia strains are slow-growing. Franczuk et al. [66] observed the growth of strains on Columbia blood agar after at least 48 h and on Löwenstein–Jensen medium after 4 days of growth. In the work of Jannat-Khah et al. [67], strains began to grow on day 3 of incubation, and active growth was observed on day 11. Iida et al. [26] cultivated Gordonia strains on Muller–Hinton agar slants for 1 week. The slow growth of Gordonia strains is a significant problem since it takes a long time to determine a correct diagnosis and begin therapy.
The strains, in most cases, have a characteristic appearance [68]. Franczuk et al. [66] observed creamy-yellowish colonies on Columbia agar, and the growth of yellow–orange colonies was noted on Löwenstein–Jensen solid medium. However, the appearance alone is insufficient to identify Gordonia strains because some Rhodococcus species may look the same.

2.2. Biochemical Test

To determine enzymatic activities, API CORYNE strips are used; however, using this method, the Gordonia strains are usually identified as Rhodococcus [57,69] or Nocardia and other actinomycetes [65].
The API CORYNE (BIOMERIEUX) system is a set of 20 micro-tubes that contain dehydrated substrates. The kit is designed to demonstrate (a) enzymatic activity and (b) the fermentation of carbohydrates. Strips for enzymatic reactions are inoculated with a concentrated suspension of microorganisms. During incubation, metabolic reactions in bacteria provoke a color change. Strips for fermentation, in turn, are inoculated with an enriched medium with a pH indicator. Fermentation reactions provoke acidification of the medium, as a result of which the color of the pH indicator changes.
In addition to enzymatic reactions, substrate utilization profiling is sometimes used. This method, along with the API CORYNE enzymatic assay, can be attributed to biological fingerprinting approaches. For substrate utilization profiling, either cultivation with the substrate is used [70] or test systems, for example, the Biolog GP2 MicroPlate assay [26]. This system is based on redox chemistry. This chemistry reacts to bacterial respiration, not the appearance of metabolites, and therefore does not need the addition of colored reagents.

3. Matrix-Assisted Laser Desorption Ionization–Time of Flight (MALDI–TOF) Mass Spectrometry (MS)

Matrix-assisted laser desorption ionization–time of flight (MALDI–TOF) mass spectrometry (MS) is an automated method recently implemented as a tool for bacterial identification in clinical microbiology laboratories [71]. This method of identifying Gordonia strains in clinical samples began to be used earlier than sequencing and currently remains in demand. Among the advantages of MALDI as a method of bacterial identification, Alcolea-Medina et al. [72] point out that it is simpler and cheaper than whole-genome sequencing (WGS).
According to the standard Bruker score system, for the identification of species, the score value must be ≥2.0, for the genus, between 2.0 and ≥1.7, and if there is a score of ≤1.7, identification is considered unreliable [73]. Due to the poor identification of Gordonia strains in accordance with generally accepted score values, some authors suggest lowering the cutoff thresholds so that they are ≥1.5 and ≥1.7 for the genus and species, respectively. Thus, Rodriguez-Lozano et al. [74] identified G. bronchialis with a score value of 1.72 (Bruker Biotyper ver. 3.1), which was lower than that defined in the manufacturer’s criteria (>2.00) for the acceptance of identification at the species level. The MALDI identification results were validated using 16S rRNA sequencing.
Similar results were previously obtained by Barberis et al. [75] when analyzing a collection of Gram-positive rods of clinical origin, including three Gordonia strains. Only one G. terrae strain was identified with a score >2.0 (Biotyper ver. 3.1). Ercibengoa Arana et al. [71] demonstrated that when the cutoff threshold is reduced to ≥1.5 and ≥1.7 for genus and species, respectively, the number of cases of successful identification of Gordonia strains increases significantly, from 10 to 20 isolates at the genus level and from 2 to 11 isolates at species level. In ref. [71], measurements were taken in three repetitions, and the average of the three results was used for further analysis.
Researchers believe that the main reason for the erroneous identification of Gordonia strains when using the MALDI method is the lack of information regarding many species in the Bruker database (Table 3).
Thus, in the work of Hsueh et al. [81], three Gordonia amicalis were mistakenly identified as G. rubripertincta because G. amicalis is not included in the Bruker Biotyper 3.1 software (database [DB] 5627). Ercibengoa Arana et al. [71] misidentified four G. otitidis isolates, probably because of the absence of any G. otitidis reference isolate in the Bruker database. Ercibengoa Arana et al. [71] used the following reference strains available in the Bruker database: Gordonia aichiensis, G. alkanivorans, G. australis, G. bronchialis (n = 2), G. rubripertincta (n = 11), and G. sputi (n = 4). The isolates studied by Lam et al. [79] and Ding et al. [40] were identified as Gordonia sp. Identification of the species was not performed because the strains did not correspond sufficiently to any species in the Bruker database (Bruker Biotyper ver. 3.1). Bzdil et al. [38] point out that MALDI Biotyper MBT 4.1 currently contains six Gordonia spp. only (G. aichiensis, G. alkanivorans, G. bronchialis, G. rubripertincta, G. sputi, and G. terrae).

4. Chromatographic Approaches

4.1. High-Performance Liquid Chromatography (HPLC)

The genera Gordonia, Nocardia, and Rhodococcus, belong to the cell wall chemotype IV. Their whole-cell sugar pattern is characterized by the presence of meso-diaminopimelic acid (meso-DAP), arabinose, and galactose in cell hydrolysates [82]. The genera of this cell wall type are classified based on the presence or absence of mycolic acids and the molecular weights of the mycolates [83,84].
Analysis of the profile of mycolic acids of Gordonia strains is sometimes used to identify them to a genus and is useful for separating Gordonia from the genera of other Actinobacteria [54]. However, previously [51], it was revealed that the mycolic acid pattern of the Gordonia strain, as assayed by HPLC, was similar to that of the Nocardia representatives. The mycolic acids of Nocardia species have 46–58 carbon atoms [83,85].
According to the profile of mycolic acids, it is possible to distinguish Gordonia from Rhodococcus. Gordonia strains have mycolic acids with 44–66 carbon atoms and dehydrogenated menaquinones with 9 isoprene units. The mycolic acids of Rhodococcus strains, on the other hand, have 34–52 carbon atoms and dehydrogenated menaquinones with 8 isoprene units [60]. The HPLC method is not suitable for the fast and accurate identification of Gordonia strains in clinical samples, especially to the species, and therefore is currently rarely used for this purpose and only together with genetic approaches.

4.2. Thin-Layer Chromatography

The thin-layer chromatography method for identifying aerobic actinomycetes was first used a long time ago [86,87]. The method consists of separating diaminopimelic acid (DAP) and sugars isolated from cells on a chromatographic plate, followed by staining of these compounds [88,89]. DAP visualization is performed by spraying a sample with 0.2% ninhydrin in acetone and heating at 100 °C for 3 min; sugar visualization is conducted by spraying the chromatogram with acid aniline phthalate and heating at 100 °C for 4 min.
TLC for identifying Gordonia by DAP and sugar was used by Aoyama et al. [90] along with 16S rRNA gene sequencing. All 31 strains were determined by TLC pattern analysis to contain N-type mycolic acid, which is characteristic of Gordonia, Nocardia, and Rhodococcus. All strains contained arabinose and galactose as characteristic components in addition to meso-DAP [91].
Hamid et al. [44] identified a Gordonia strain isolated from a Zebu cow with lymphadenitis. Among the approaches used were TLC, 16S rRNA gene sequencing, and DNA–DNA hybridization. On thin-layer chromatography, the organism contained mycolic acids that co-chromatographed with mycolates from Gordonia species. The strain was determined as G. sinesedis with the help of genetic methods.
TLC is not a method accurate enough to identify strains to species based on its results. In addition, it does not meet modern requirements for the rapidity of analysis, and labor costs are inferior to other methods, particularly genetic ones. In this regard, TLC is now rarely used in clinical practice, as well as HPLC.

5. Genetic Approaches

5.1. Amplification and Sequencing of Phylogenetic Markers

Despite the spread of genetic methods for identifying microorganisms in various fields of biological science and industries, these methods have been used in medicine relatively recently. Identifying Gordonia strains in clinical samples by sequencing the main phylogenetic markers and analyzing the results has only become widely used in the last 10–15 years [52,54,69].
As phylogenetic markers for identifying microorganisms, housekeeping genes are usually used. Housekeeping genes are necessary to maintain the most important vital functions of the organism. The housekeeping genes most commonly used as phylogenetic markers are as follows: 16S rRNA, gyrB, rpoB, cat, and ppk [92]. The sequencing and analysis of additional phylogenetic markers, i.e., more specific genes that are not housekeeping, is a more specific task and mainly serves to distinguish closely related species within species groups [93]. Specific phylogenetic markers are not used to identify Gordonia in clinical samples.

5.1.1. 16S rRNA

The most commonly used phylogenetic marker for identifying Gordonia is the 16S rRNA gene because it contains both highly conserved and hypervariable regions [94]. In addition, the advantage of using this gene as a marker is that reference databases have been compiled for analysis [95,96,97,98].
To identify the Gordonia strains, both an almost complete gene and only variable regions are sequenced. In the work of Franczuk et al. [66], which aimed to identify G. bronchialis, the V3-V4 region of the 16S rRNA gene was amplified with the use of primer “forward” 5′-ACTCCTACGGGAGGCAGCAG-3′ and primer “reverse” 5′-TACCAGGGTATCTAATCC-3′. Wang et al. [99] performed rapid metagenomic next-generation sequencing of 16S rRNA to determine G. aichiensis in a patient with peritoneal dialysis-associated peritonitis.
However, in most cases, sequencing the longest possible fragment of the 16S rRNA gene of individual isolates is performed (Table 4).
At the same time, 16S rRNA amplicon sequencing has several disadvantages:
  • Since the 16S rRNA gene is very conservative and evolves extremely slowly, it cannot be used to separate closely related strains and identify them.
  • During the amplification of 16S rRNA, the formation of chimeric amplicons is possible [109,110].
  • The number of copies of the 16S rRNA gene in different species is variable, and single-nucleotide polymorphisms (SNPs) at the single-cell level may result in an overestimation of diversity [111].
  • In the case of closely related species, it is difficult to delineate species in cluster analysis [112].
Due to the above-mentioned features of the use of the 16S rRNA gene for identifying microorganisms, in some cases, it is necessary to use additional phylogenetic markers. In the case of Gordonia strains, the gyrB, secA, and hsp65 genes are most often used [50,79,105].

5.1.2. gyrB (gyrase B)

The threshold for assigning bacteria to a species based on the gyrB sequence is lower than 16S rRNA. This is due to the greater variability of the gyrB gene relative to 16S rRNA. Currently, for gyrB phylogeny, the species threshold is not clearly marked; it is different for different groups of organisms [113]. According to Kang et al. [114], the species threshold for Gordonia is 77.5–97.6%.
DNA gyrase plays an important role in DNA replication [115]. Both A and B subunits of DNA gyrase can be used as phylogenetic markers. Thus, gyrA is often used to identify bacilli [116,117]. However, we have not found any examples of the use of gyrA as a marker for the identification of Gordonia strains in the literature. Perhaps the preferred use of gyrB for this purpose is due to a more meticulous methodological base (primers and amplification modes) and a large number of reference sequences of Gordonia gyrB with which the data obtained can be compared in databases.
Shen et al. [118] identified Gordonia strains using gyrB and 16S rRNA gene sequences. A pair of primers for the amplification of the gyrB gene was developed using conserved amino acid sequences MTQLHAG and KLRYHKIV of E. coli DNA gyrase (Table 5). The GYRB1 sequence has a single amino acid replacement in comparison with the primer UP-1 from the UP-1/UP-2 pair [119,120], which are the most commonly used classical primers for the amplification of gyrB. The reverse primer was newly designed.
In the work of Jannat-Khah [67], the Gordonia araii strain was identified by gyrB sequencing. This is the first case of detecting a pathogenic strain of G. araii causing infection associated with a medical device. For gyrB gene amplification, the primer pair GYRB1/GYRB2 [118] was used.
Johnson et al. [121], using sequencing and analysis of 16S rRNA and gyrB genes, identified G. bronchialis in isolates obtained from a 52-year-old woman with a history of Hodgkin’s lymphoma, prior splenectomy, and breast cancer. For the amplification of the gyrB gene, the primer pair GYRB1/GYRB2 [118] was used. Both patient isolates were 100% similar and 93% related to the type strain of G. bronchialis. Similarly, G. bronchialis was identified in the work of Akrami et al. [65] in a 69-year-old man with erythema and drainage at the cranial end of the sternotomy incision. PCR amplification of the DNA gyrase region of Gordonia spp. was carried out with a set of novel PCR primers; however, the primer sequences were not specified.
The strains of Gordonia species that rarely cause human infections are also known to be identified using gyrB. So, Ding et al. [40] identified Gordonia polyisoprenivorans as a cause of catheter-related bacteremia in an AIDS patient. Sequencing of the gyrB genes was performed according to a previous report [6] using the GYRB1/GYRB2 primer pair.
Negishi et al. [105] found G. sputi in a sample from an 18-year-old man with acute lymphocytic leukemia. Here, identification was also performed using two markers, 16S rRNA and gyrB; however, here, unlike the works mentioned above with gyrB, amplification was performed not with GYRB1/GYRB2 primers but according to the work of Kang et al. [114]. Authors revealed that G. sputi could not be distinguished from G. aichiensis or G. otitidis using 16S rRNA gene sequence analysis alone but could be successfully discriminated against using the gyrB gene sequence.
Kang et al. [114], for gyrB amplification, used both primers UP [120] and the F1/R1296 pair, as well as the gyrB sequence of Nocardia farcinica IFM 10152 [122]. The primer F1 is a modified and more specific version of UP1. Later, the F1/R1296 pair was used for the amplification of gyrB of Nocardia [123]. Modified primers UP are also known [50]; they were used to identify G. otitidis in the sputum sample taken from a 76-year-old woman suspected of having nontuberculous mycobacterial (NTM) lung disease. For the sequencing of the amplicon primers, sF1 (5′-GAG GTC GTC ATG ACC CAG CTG CA-3′) and sR1296-modi (5′-AGC AGC GTC GAG ATG TGC TGG CC-3′) were used.
Among the disadvantages of using gyrB as a phylogenetic marker, Kang et al. [114] mention that gyrases of not all Gordonia species can be amplified using a pair of F1/R1296 primers. A similar drawback was also noted in the UP pair [118]. Currently, the most commonly used pair of primers for identifying Gordonia in clinical samples is GYRB1/GYRB2.
Another disadvantage of using gyrB as a phylogenetic marker is establishing similarity cutoff criteria for reliable and accurate identification since intraspecies sequence variability has been observed [124]. Authors cite the heterogeneous species Gordonia terrae, where the similarity of different strains with type one can vary at 87–98%. Authors suggest that in the case of heterogeneous species, other (non-gyrB) phylogenetic markers and DNA–DNA hybridization may be useful for identification.

5.1.3. secA, hsp65

In some cases, secA, not gyrB, is used to identify clinical samples of Gordonia in addition to 16S rRNA. SecA is an ATPase that plays an essential role in the protein translocation mechanism [125,126]. Both gyrB and secA provide a greater discrimination degree compared to 16S rRNA. According to Lasker et al. [124], interspecies sequence similarity for the secA gene sequence and the SecA amino acid sequence was 81.9–98.0% and 83.0–100.0%, respectively. The amino acid motif constructed based on the secA1 amino acid sequences provides the opportunity to discriminate the genus Gordonia from related pathogenic actinomycetes such as Nocardia, Streptomyces, and Mycobacterium [114].
Lam et al. [79] used secA as an additional (in addition to 16S rRNA) marker for identifying Gordonia strains in samples taken from four patients with continuous ambulatory peritoneal dialysis-related peritonitis. For amplification, a pair of SecA1-f/SecA1-r (Table 6) primers [114] was used. These primers were developed using data regarding the gene sequences of Mycobacterium and Nocardia in GenBank [127,128]. The sequencing and analysis of 16S rRNA and secA amplicons successfully identified G. sputi in two patients and G. bronchialis in one patient. As for the isolate detected in the fourth patient, its 16S rRNA gene had 99.7% identity to that of the Gordonia terrae type strain, but the secA1 gene had 94.0% sequence identity to that of the Gordonia lacunae type strain. The authors suggested that it was a novel Gordonia species [79].
Given the difficulties in identifying individual Gordonia isolates even when using two markers, several researchers propose a multilocus analysis of at least three markers. The most commonly used combination is 16S rRNA, gyrB, and secA. For the first time, this approach was used by Kang et al. [114]. The authors noted that sometimes there was no signal during the amplification of gyrB in some species using primers that were successfully used for other species. The length of the gyrB amplicons during amplification with the same primers turned out to be different: in most Gordonia, it was 1230 bp, and in G. otitidis, 1188 bp.
Using the third marker (secA) solved the problem with gyrB. Universal primers have been developed to amplify the 496 bp region of the secA1 gene (Table 4).
Kim et al. [50], to identify nontuberculous mycobacteria (NTM) in the sputum sample taken from a woman with lung disease, used genotypic identification targeting an internal transcribed spacer (ITS). The strain was determined by this method as Mycobacterium lenti-flavum or Mycobacterium genavense. However, sequencing of 16S rRNA, gyrB, and secA1 genes revealed that the strain belonged to G. otitidis. In this regard, it can be concluded that the method convenient for mycobacteria is not suitable for Gordonia.
There are known examples of identifying Gordonia by analyzing the 441 bp fragment (Telenti segment) of the hsp65 gene [129]. This method was first proposed by Telenti et al. [130] and is widely used for identifying mycobacteria [131,132], but it is used infrequently for Gordonia. Unlike the phylogenetic markers described above, for which the main stages of work consisted of amplification and sequencing, in the case of hsp65, restriction analysis is assumed.
Lai et al. [103] analyzed the strains of Gordonia, which were the causative agents of infections, at a medical center in Taiwan from 1997 to 2008. To identify the strains, the authors used 16S rRNA gene sequence analysis and restriction profiles of the 440 bp fragment of the 65 kDa heat shock protein gene (hsp65) amplified using the primers TB11 (5′-ACCAACGATGGTGTGTCCAT-3′) and TB12 (5′-CTTGTCGAACCGCATACCCT-3′) [129,133]. Hydrolysis of amplicons was performed with the help of enzymes MspI and HinfI. Using this method, G. terrae and G. sputi were identified. Chang et al. [77] and Wright et al. [101], using 16S rRNA and hsp65, identified G. bronchialis in a case of deep sternal wound infection with sternal osteomyelitis after open-heart surgery.
In addition to housekeeping gene analysis (16S rRNA, hsp65), Lai et al. [103] used random amplified polymorphic DNA (RAPD) analysis performed using primers M13 (5′-TTATGTAAAACGACGGCCAGT-3′) and H4 (5′-GGAAGTCGCC-3′). The isolates from different patients had different patterns, indicating that they were genetically unrelated, and that nosocomial transmission had not occurred. In this paper, RAPD analysis was used for the first time to study the clinical isolates of Gordonia.

5.2. DNA–DNA Hybridization

Among the genetic methods not related to sequencing, DNA–DNA hybridization can be noted. The use of hybridization for species identification is rational when the number of candidate species is reduced by other methods to 1–2; otherwise, the approach becomes methodical and time-consuming. Verma et al. [54] identified G. polyisoprenivorans in a blood sample of a 78-year-old male with a medical history of multiple episodes of gastrointestinal bleeding secondary to Osler–Weber–Rendu and myelodysplastic syndrome with pancytopenia. The authors used 16S rRNA gene sequencing and DNA–DNA hybridization. G. polyisoprenivorans are infrequent human pathogens. Usually, these are soil strains that, due to their ability to recycle rubber, have the potential for use in biotechnology [134]. However, it is known that G. polyisoprenivorans strains can form biofilms on the catheter surface [59,135,136].
DNA–DNA hybridization was used by Jannat-Khah et al. [67] to confirm the results obtained by sequencing the 16S rRNA and gyrB genes. The high degree of sequence similarity (99.6%) between the 16S rRNA gene sequences for isolate W8543 and the G. araii type strain allowed them to identify the isolate as G. araii, and DNA–DNA hybridization analysis supported the results.

5.3. Next-Generation Sequencing (NGS) for Gordonia Identification

The Gordonia strains continue to be considered rare pathogens, but the problem of identifying these strains in clinical samples remains unresolved. Multilocus sequencing of amplicons currently remains the most accurate of the methods used for the taxonomic determination of strains; however, it takes time, and, in addition, there is always a possibility that the selected amplification mode will not work for a particular sample.
Sequencing whole genomes is a promising method for the rapid and accurate identification of Gordonia strains. At the same time, replenishing databases with genomes of Gordonia, including genomes belonging to clinical strains, will make it possible to operate with more material for genome comparison in the future.
When identifying strains based on the whole genome sequence, modern in silico methods, such as digital hybridization (DDH), can be used [137]. If the genomic DNA of two organisms reveals a DDH similarity of below 70%, these strains are considered representatives of distinct species and vice versa [138,139].
There are few examples of sequencing genomes of pathogenic Gordonia in modern literature. Koenigsaecker et al. [140] sequenced the strain Gordonia sp. UCD-TK1 isolated from a patient chair in a surgery center (Redding, CA, USA). The genome was sequenced on Illumina MiSeq (2 × 300) and assembled using an A5 assembler [141] to 95 scaffolds with 22× coverage. The greatest similarity in the 16S rRNA gene was observed with representatives of G. terrae and G. lacunae. However, the authors did not carry out the definition of the species due to the lack of data on the complete genomes of other representatives of G. lacunae, which could be used as a reference.
Gulvik et al. [142] sequenced the Gordonia sp. strain X0973 obtained from a human abscess. The authors used Illumina MiSeq and PacBio reads to obtain complete assembly. As a result, a complete circular genome sequence of 3.75 Mbp was obtained. Initially, the strain was identified as Gordonia by 16S rRNA gene sequencing and previously assigned to the species G. amarae. It is further stated that the average nucleotide identity (ANI) of the isolate with Gordonia type strains is in the range of 80.9 ± 5.4%, and DDH with Gordonia araii type strain (which is considered as the closest relative) is 22.6%. Such a conclusion is somewhat unusual, given that the species threshold for DDH is at least 70% [137].
Bzdil et al. [38] studied a variety of Gordonia strains isolated from the milk of dairy cows with mastitis. Nine isolates were identified as G. paraffinivorans by whole-genome sequencing. An interesting fact is that there are no examples of the pathogenic effects of G. paraffinivorans on humans in the literature; however, in veterinary medicine, there are several other reported infections caused by this genus. G. paraffinivorans, similar to G. polyisoprenivorans, is primarily interesting as a promising biotechnological agent for the degradation of hydrocarbon pollutants and is rarely the cause of diseases. Ahrholdt [143] revealed G. paraffinivorans as a cause of mastitis in cows in Saxony, Germany. Similar work was performed by Valkó [144] in Hungary, where the representatives of G. paraffinivorans caused the same disease in cows. In both cases, pathogens were identified by the sequencing and analysis of 16S rRNA genes.
In all nine samples, the authors [38] identified genes encoding virulence factors similar to those of Mycobacterium tuberculosis and Mycobacterium smegmatis. However, the authors noted that five genes similar to the virulence genes of Mycobacterium were found in the genome of the isolates from mastitis cases and both environmental reference strains. From the results obtained, it can be assumed that the pathogenicity or non-pathogenicity of strains is not so much due to the presence of certain genes as the expression of these genes. This assumption may be supported by the fact that there are not only pathogenic or non-pathogenic species among Gordonia; in each case, we are talking about specific representatives.

6. Treatment of Diseases Caused by Gordonia Strains

Infections caused by Gordonia spp. are often difficult to diagnose [49]. This is due to erroneous identification using a phenotypic test and slow growth of strains (approximately 3 days). The biochemical analysis used to determine the species is often unreliable [1]. However, most infections are resolved after the removal of the infected medical device and antibiotic treatment, resulting in the successful recovery of the patients [25]. The main advantage of this approach is that Gordonia, unlike related actinobacteria, does not have multiple antibiotic resistance [38,52]. The disadvantage is that there is no single treatment regimen for infections of Gordonia strains, and for each case, treatment must be selected.
Sometimes antibiotic therapy is prescribed to the patient empirically, according to symptoms, without waiting to identify the pathogen organism and determine the spectrum of antibiotic resistance. For example, in the work of Brust et al. [63], one of the patients was initially started on vancomycin and piperacillin/tazobactam, but this was changed to imipenem, amikacin, and minocycline, and the results of determining the strain as G. sputi were obtained when the therapy had already been started. A similar approach was used by Ramanan et al. [53] and Negishi et al. [105].
There are cases when, due to the erroneous definition of Gordonia as Nocardia, Mycobacterium, etc., the treatment was ineffective. Thus, trimethoprim–sulfamethoxazole is often used to treat Nocardia infections [145], and Blaschke et al. [52] show that it is ineffective against Gordonia.
Jeong Rae et al. [55] mistakenly identified the pathogen strain by biochemical methods as Corynebacterium, and treatment was selected in accordance with the approaches adopted for Corynebacterium strains: the authors used vancomycin, ceftriaxone, and clindamycin combination, and piperacillin/tazobactam, but the patient’s condition did not improve, and only after that the authors used 16S rRNA gene sequencing to identify the strain as Gordonia.
Martin et al. [78] suspected Listeria monocytogenes infection in a patient (by biochemical and microbiological examination of cerebrospinal fluid). The treatment was selected based on experience with Listeria: ampicillin, associated with vancomycin and ceftriaxone. However, the patient persisted with fever, and therapy was changed to linezolid and meropenem to cover the possibility of nosocomial secondary infection [78]. After, the pathogen strain was identified correctly (Gordonia sputi) using the MALDI TOF MS method.
The correct identification of the pathogenic organism to the species will allow, first, not to waste time on therapy designed for other groups of organisms and ineffective for Gordonia. Second, it will make it possible to use the experience of predecessors to successfully choose antibiotics for various species of Gordonia. Parallel to the identification of the microorganism, clinicians usually carry out antibiotic resistance testing. Most of the known Gordonia strains are susceptible to amoxicillin-clavulanate, amikacin, ceftriaxone, ciprofloxacin, linezolid, meropenem, minocycline, trimethoprim-sulfamethoxazole, tigecycline, and vancomycin [57,67,121]. At the same time, Moser et al. [136] revealed that the G. polyisoprenivorans strain had poor susceptibility to trimethoprim-sulfamethoxazole, clarithromycin, tigecycline, and minocycline. In ref. [65], the strain of G. bronchialis was susceptible to penicillin, gentamicin, levofloxacin, minocycline, vancomycin, linezolid, tetracycline, and erythromycin. It can therefore be concluded that despite the lack of a universal approach to the treatment of Gordonia infections, there is still some information regarding the use of antibiotics against different Gordonia species.
It is known that G. otitidis can be successfully treated with meropenem and ceftriaxone [68], imipenem, and clarithromycin [52]. Vancomycin is used against G. terrae [146], sometimes in combination with ceftazidime [147] or rifampin [52], as well as ciprofloxacin [52]. Treatment of G. polyisoprenivorans infections is often achieved using imipenem, ciprofloxacin, and vancomycin [40,54]. We believe that selecting effective antibiotics without the need for a “trial-and-error” approach will avoid the appearance of multidrug resistance in Gordonia in the future.

7. Prospects for Working with Infections Caused by Gordonia Strains

Recent studies show that the problem of identifying Gordonia strains in clinical samples remains unresolved. Based on the works reviewed, the following trends in this field can be formulated:
  • Chromatographic methods and mass spectrometry are currently rarely used to identify Gordonia strains. Chromatographic methods fail to distinguish them from related genera (Nocardia and Rhodococcus).
  • Currently, MALDI–TOF MS is the main instrument for identifying Gordonia in clinical samples. The accuracy of this method in detecting the genus is proven, but MALDI–TOF MS is unsuitable for accurately identifying Gordonia as a species.
  • The analysis for antibiotic resistance is necessary to accumulate information regarding the resistance/sensitivity of different Gordonia species to antibiotics. Depending on this information, the treatment of infections caused by each species of Gordonia is selected.
  • At the moment, the most accurate identification result can be obtained either by multilocus sequencing of housekeeping genes (16S rRNA, gyrB, and secA) or by whole-genome sequencing. There is reason to believe that these methods will become increasingly widespread.
The correct determination of the taxonomic position of strains allows, on the one hand, to quickly select effective therapy based on the experience of predecessors and, on the other, to replenish the pool of methodological approaches to treat Gordonia infections of different species.

8. Conclusions

Gordonia spp. are common environmental bacteria with flexible genome structures and diverse metabolic capabilities. Despite their attractiveness for use in various fields of biotechnology, researchers are increasingly concerned about the growing number of clinical cases of infection with Gordonia strains, especially in immunocompromised patients. The main problems of working with Gordonia in medicine today are the complexity of their rapid and accurate identification and the lack of a universal therapy regimen.
The cases analyzed reveal the importance of molecular analysis in the definitive identification of these and other related species. The spread of genetic methods of identification of Gordonia strains suggests that in the near future, it will be possible to solve the problem of the erroneous identification of these strains.

Author Contributions

Conceptualization, Y.D. and A.B.; formal analysis, A.V.; writing—original draft preparation, Y.D. and E.F.; writing—review and editing, Y.D., A.B. and A.V.; project administration, Y.D.; funding acquisition, Y.D. All authors have read and agreed to the published version of the manuscript.

Funding

This work was financially supported by the Russian Science Foundation, grant number 22-74-10082.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Andalibi, F.; Fatahi-Bafghi, M. Gordonia: Isolation and identification in clinical samples and role in biotechnology. Folia Microbiol. 2017, 62, 245–252. [Google Scholar] [CrossRef]
  2. Delegan, Y.A.; Valentovich, L.N.; Shafieva, S.M.; Ganbarov, K.G.; Filonov, A.E.; Vainstein, M.B. Characterization and genomic analysis of highly efficient thermotolerant oil-degrading bacterium Gordonia sp. 1D. Folia Microbiol. 2019, 64, 41–48. [Google Scholar] [CrossRef] [PubMed]
  3. Kubota, K.; Koma, D.; Matsumiya, Y.; Chung, S.-Y.; Kubo, M. Phylogenetic analysis of long-chain hydrocarbon-degrading bacteria and evaluation of their hydrocarbon-degradation by the 2,6-DCPIP assay. Biodegradation 2008, 19, 749–757. [Google Scholar] [CrossRef]
  4. Wang, X.; Jin, D.; Zhou, L.; Wu, L.; An, W.; Zhao, L. Draft Genome Sequence of Gordonia alkanivorans Strain CGMCC6845, a Halotolerant Hydrocarbon-Degrading Bacterium. Genome Announc. 2014, 2, e01274-13. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. Kurniati, T.H.; Rusmana, I.; Suryani, A.; Mubarik, N.R. Degradation of Polycyclic Aromatic Hydrocarbon Pyrene by Biosurfactant-Producing Bacteria Gordonia cholesterolivorans AMP 10. Biosaintifika J. Biol. Biol. Educ. 2016, 8, 336. [Google Scholar] [CrossRef] [Green Version]
  6. Lin, C.-L.; Shen, F.-T.; Tan, C.-C.; Huang, C.-C.; Chen, B.-Y.; Arun, A.B.; Young, C.-C. Characterization of Gordonia sp. strain CC-NAPH129-6 capable of naphthalene degradation. Microbiol. Res. 2012, 167, 395–404. [Google Scholar] [CrossRef] [PubMed]
  7. Mai, Z.; Wang, L.; Li, Q.; Sun, Y.; Zhang, S. Biodegradation and metabolic pathway of phenanthrene by a newly isolated bacterium Gordonia sp. SCSIO19801. Biochem. Biophys. Res. Commun. 2021, 585, 42–47. [Google Scholar] [CrossRef]
  8. Aminsefat, A.; Rasekh, B.; Ardakani, M.R. Biodesulfurization of dibenzothiophene by Gordonia sp. AHV-01 and optimization by using of response surface design procedure. Microbiology 2012, 81, 154–159. [Google Scholar] [CrossRef]
  9. Delegan, Y.; Kocharovskaya, Y.; Frantsuzova, E.; Streletskii, R.; Vetrova, A. Characterization and genomic analysis of Gordonia alkanivorans 135, a promising dibenzothiophene-degrading strain. Biotechnol. Rep. 2021, 29, e00591. [Google Scholar] [CrossRef]
  10. Kim, S.B.; Brown, R.; Oldfield, C.; Gilbert, S.C.; Iliarionov, S.; Goodfellow, M. Gordonia amicalis sp. nov.; a novel dibenzothiophene-desulphurizing actinomycete. Int. J. Syst. Evol. Microbiol. 2000, 50, 2031–2036. [Google Scholar] [CrossRef]
  11. Wang, W.; Ma, T.; Lian, K.; Zhang, Y.; Tian, H.; Ji, K.; Li, G. Genetic Analysis of Benzothiophene Biodesulfurization Pathway of Gordonia terrae Strain C-6. PLoS ONE 2013, 8, e84386. [Google Scholar] [CrossRef] [Green Version]
  12. Andler, R.; Hiessl, S.; Yücel, O.; Tesch, M.; Steinbüchel, A. Cleavage of poly(cis-1,4-isoprene) rubber as solid substrate by cultures of Gordonia polyisoprenivorans. New Biotechnol. 2018, 44, 6–12. [Google Scholar] [CrossRef]
  13. Bröker, D.; Arenskotter, M.; Legatzki, A.; Nies, D.H.; Steinbüchel, A. Characterization of the 101-Kilobase-Pair Megaplasmid pKB1, Isolated from the Rubber-Degrading Bacterium Gordonia westfalica Kb1. J. Bacteriol. 2004, 186, 212–225. [Google Scholar] [CrossRef] [Green Version]
  14. Linos, A.; Berekaa, M.M.; Steinbüchel, A.; Kim, K.K.; Sproer, C.; Kroppenstedt, R.M. Gordonia westfalica sp. nov., a novel rubber-degrading actinomycete. Int. J. Syst. Evol. Microbiol. 2002, 52, 1133–1139. [Google Scholar] [CrossRef] [Green Version]
  15. Arenskötter, M.; Linos, A.; Schumann, P.; Kroppenstedt, R.M.; Steinbüchel, A. Gordonia nitida Yoon et al. 2000 is a later synonym of Gordonia alkanivorans Kummer et al. 1999. Int. J. Syst. Evol. Microbiol. 2005, 55, 695–697. [Google Scholar] [CrossRef]
  16. Franzetti, A.; Caredda, P.; la Colla, P.; Pintus, M.; Tamburini, E.; Papacchini, M.; Bestetti, G. Cultural factors affecting biosurfactant production by Gordonia sp. BS29. Int. Biodeterior. Biodegrad. 2009, 63, 943–947. [Google Scholar] [CrossRef]
  17. Zargar, A.N.; Mishra, S.; Kumar, M.; Srivastava, P. Isolation and chemical characterization of the biosurfactant produced by Gordonia sp. IITR100. PLoS ONE 2022, 17, e0264202. [Google Scholar] [CrossRef]
  18. Morikawa, M.; Hirata, Y.; Imanaka, T. A study on the structure–function relationship of lipopeptide biosurfactants. Biochim. Et Biophys. Acta (BBA) Mol. Cell Biol. Lipids 2000, 1488, 211–218. [Google Scholar] [CrossRef]
  19. Moormann, M.; Zähringer, U.; Moll, H.; Kaufmann, R.; Schmid, R.; Altendorf, K. A New Glycosylated Lipopeptide Incorporated into the Cell Wall of a Smooth Variant of Gordona hydrophobica. J. Biol. Chem. 1997, 272, 10729–10738. [Google Scholar] [CrossRef] [Green Version]
  20. Silva, T.P.; Paixão, S.M.; Tavares, J.; Gil, C.V.; Torres, C.A.V.; Freitas, F.; Alves, L. A New Biosurfactant/Bioemulsifier from Gordonia alkanivorans Strain 1B: Production and Characterization. Processes 2022, 10, 845. [Google Scholar] [CrossRef]
  21. Fernandes, A.S.; Paixão, S.M.; Silva, T.P.; Roseiro, J.C.; Alves, L. Influence of culture conditions towards optimal carotenoid production by Gordonia alkanivorans strain 1B. Bioprocess Biosyst. Eng. 2018, 41, 143–155. [Google Scholar] [CrossRef] [PubMed]
  22. Kwon, S.J.; Choi, Y.J.; Kim, J.M.; Lee, P.C. Complete Genome Sequence of the Carotenoid-Producing Strain Gordonia ajoucoccus A2. Microbiol. Resour. Announc. 2020, 9, e00662-20. [Google Scholar] [CrossRef] [PubMed]
  23. Lee, K.-W.; How, C.W.; Chen, L.; Chen, P.T.; Lan, J.C.-W.; Ng, H.-S. Integrated extractive disruption of Gordonia terrae cells with direct recovery of carotenoids using alcohol/salt aqueous biphasic system. Sep. Purif. Technol. 2019, 223, 107–112. [Google Scholar] [CrossRef]
  24. Loh, W.L.C.; Huang, K.-C.; Ng, H.S.; Lan, J.C.-W. Exploring the fermentation characteristics of a newly isolated marine bacteria strain, Gordonia terrae TWRH01 for carotenoids production. J. Biosci. Bioeng. 2020, 130, 187–194. [Google Scholar] [CrossRef] [PubMed]
  25. Drzyzga, O. The strengths and weaknesses of Gordonia: A review of an emerging genus with increasing biotechnological potential. Crit. Rev. Microbiol. 2012, 38, 300–316. [Google Scholar] [CrossRef]
  26. Iida, S.; Taniguchi, H.; Kageyama, A.; Yazawa, K.; Chibana, H.; Murata, S.; Nomura, F.; Kroppenstedt, R.M.; Mikami, Y. Gordonia otitidis sp. nov.; isolated from a patient with external otitis. Int. J. Syst. Evol. Microbiol. 2005, 55, 1871–1876. [Google Scholar] [CrossRef] [Green Version]
  27. Kageyama, A.; Iida, S.; Yazawa, K.; Kudo, T.; Suzuki, S.; Koga, T.; Saito, H.; Inagawa, H.; Wada, A.; Kroppenstedt, R.M.; et al. Gordonia araii sp. nov. and Gordonia effusa sp. nov.; isolated from patients in Japan. Int. J. Syst. Evol. Microbiol. 2006, 56, 1817–1821. [Google Scholar] [CrossRef]
  28. Kang, Y.-Q.; Ming, H.; Gonoi, T.; Chen, Y.; Cao, Y.; Wang, Y.-Y.; Cheng, J.; Koga, T.; Mikami, Y.; Li, W.-J. Gordonia iterans sp. nov.; isolated from a patient with pneumonia. Int. J. Syst. Evol. Microbiol. 2014, 64, 3520–3525. [Google Scholar] [CrossRef] [Green Version]
  29. Klatte, S.; Rainey, F.A.; Kroppenstedt, R.M. Transfer of Rhodococcus aichiensis Tsukamura 1982 and Nocardia amarae Lechevalier and Lechevalier 1974 to the Genus Gordona as Gordona aichiensis comb. nov. and Gordona amarae comb. nov. Int. J. Syst. Bacteriol. 1994, 44, 769–773. [Google Scholar] [CrossRef] [Green Version]
  30. Tsukamura, M. Proposal of a New Genus, Gordona, for Slightly Acid-fast Organisms Occurring in Sputa of Patients with Pulmonary Disease and in Soil. J. Gen. Microbiol. 1971, 68, 15–26. [Google Scholar] [CrossRef]
  31. Renvoise, A.; Harle, J.-R.; Raoult, D.; Roux, V. Gordonia sputi Bacteremia. Emerg. Infect. Dis. 2009, 15, 1535–1537. [Google Scholar] [CrossRef]
  32. Li, S.-H.; Jin, Y.; Cheng, J.; Park, D.-J.; Kim, C.-J.; Hozzein, W.N.; Wadaan, M.A.M.; Shu, W.-S.; Ding, L.-X.; Li, W.-J. Gordonia jinhuaensis sp. nov.; a novel actinobacterium, isolated from a VBNC (viable but non-culturable) state in pharmaceutical wastewater. Antonie Van Leeuwenhoek 2014, 106, 347–356. [Google Scholar] [CrossRef] [PubMed]
  33. Yang, Z.; Zhang, Z.; Chen, M.; Liu, Z. Gordonia crocea sp. nov. Isolated from Wound Infection After Pacemaker Implantation: Case Report and Literature Review. Infect. Drug Resist. 2022, 15, 2915–2920. [Google Scholar] [CrossRef]
  34. Tsang, C.-C.; Xiong, L.; Poon, R.W.S.; Chen, J.H.K.; Leung, K.-W.; Lam, J.Y.W.; Wu, A.K.L.; Chan, J.F.W.; Lau, S.K.P.; Woo, P.C.Y. Gordonia hongkongensis sp. nov., isolated from blood culture and peritoneal dialysis effluent of patients in Hong Kong. Int. J. Syst. Evol. Microbiol. 2016, 66, 3942–3950. [Google Scholar] [CrossRef]
  35. Lai, C.-C.; Hsieh, J.-H.; Tsai, H.-Y.; Liao, C.-H.; Hsueh, P.-R. Cutaneous Infection Caused by Gordonia amicalis after a Traumatic Injury. J. Clin. Microbiol. 2012, 50, 1821–1822. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  36. Guiraud, J.; Lescure, M.; Faganello, D.; Bébéar, C.; Pereyre, S.; Ménard, A. A case of prosthetic joint septic arthritis caused by Gordonia jacobaea. J. Microbiol. Immunol. Infect. 2022, 55, 355–357. [Google Scholar] [CrossRef] [PubMed]
  37. De Miguel, T.; Sieiro, C.; Poza, M.; Villa, T.G. Isolation and taxonomic study of a new canthaxanthin-containing bacterium, Gordonia jacobaea MV-1 sp. nov. Int. Microbiol. Off. J. Span. Soc. Microbiol. 2000, 3, 107–111. [Google Scholar]
  38. Bzdil, J.; Slosarkova, S.; Fleischer, P.; Matiasovic, J. Gordonia species as a rare pathogen isolated from milk of dairy cows with mastitis. Sci. Rep. 2022, 12, 6028. [Google Scholar] [CrossRef]
  39. Xue, Y.; Sun, X.; Zhou, P.; Liu, R.; Liang, F.; Ma, Y. Gordonia paraffinivorans sp. nov., a hydrocarbon-degrading actinomycete isolated from an oil-producing well. Int. J. Syst. Evol. Microbiol. 2003, 53, 1643–1646. [Google Scholar] [CrossRef]
  40. Ding, X.; Yu, Y.; Chen, M.; Wang, C.; Kang, Y.; Li, H.; Lou, J. Bacteremia due to Gordonia polyisoprenivorans: Case report and review of literature. BMC Infect. Dis. 2017, 17, 1–4. [Google Scholar] [CrossRef] [Green Version]
  41. Linos, A.; Steinbüchel, A.; Spröer, C.; Kroppenstedt, R.M. Gordonia polyisoprenivorans sp. nov., a rubber-degrading actinomycete isolated from an automobile tyre. Int. J. Syst. Evol. Microbiol. 1999, 49, 1785–1791. [Google Scholar] [CrossRef]
  42. Hart, D.H.L.; Andrew, J.H.; Peel, M.M.; Burdon, J.G.W. Lung infection caused by rhodococcus. Aust. New Zealand J. Med. 1988, 18, 790–791. [Google Scholar] [CrossRef] [PubMed]
  43. Stackebrandt, E.; Rainey, F.A.; Ward-Rainey, N.L. Proposal for a New Hierarchic Classification System, Actinobacteria classis nov. Int. J. Syst. Bacteriol. 1997, 47, 479–491. [Google Scholar] [CrossRef] [Green Version]
  44. Hamid, M.; Musa, M.; El-Sanousi, S.; Hassan, M.; Joseph, M.; Goodfellow, M. Characterization of Gordonia sinesedis Isolated from a Zebu Cow Suffering from Lymphadenitis. Br. Microbiol. Res. J. 2015, 5, 216–226. [Google Scholar] [CrossRef] [Green Version]
  45. Maldonado, L.A.; Stainsby, F.M.; Ward, A.C.; Goodfellow, M. Gordonia sinesedis sp. nov., a novel soil isolate. Antonie Van Leeuwenhoek 2003, 83, 75–80. [Google Scholar] [CrossRef]
  46. Gil-Sande, E.; Brun-Otero, M.; Campo-Cerecedo, F.; Esteban, E.; Aguilar, L.; García-de-Lomas, J. Etiological Misidentification by Routine Biochemical Tests of Bacteremia Caused by Gordonia terrae Infection in the Course of an Episode of Acute Cholecystitis. J. Clin. Microbiol. 2006, 44, 2645–2647. [Google Scholar] [CrossRef] [Green Version]
  47. Stackebrandt, E.; Smida, J.; Collins, M.D. Evidence of phylogenetic heterogeneity within the genus Rhodococcus: Revival of the genus Gordona (Tsukamura). J. Gen. Appl. Microbiol. 1988, 34, 341–348. [Google Scholar] [CrossRef] [Green Version]
  48. Gueneau, R.; Blanchet, D.; Rodriguez-Nava, V.; Bergeron, E.; Soulier, M.; Bestandji, N.; Demar, M.; Couppie, P.; Blaizot, R. Actinomycetoma caused by Gordonia westfalica: First reported case of human infection. New Microbes New Infect. 2020, 34, 100658. [Google Scholar] [CrossRef]
  49. Fang, W.; Li, J.; Cui, H.-S.; Jin, X.; Zhai, J.; Dai, Y.; Li, Y. First identification of Gordonia sputi in a post-traumatic endophthalmitis patient—A case report and literatures review. BMC Ophthalmol. 2017, 17, 190. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  50. Kim, H.; Kim, Y.S.; Kim, K.-H.; Kim, N.; Kim, H.H.; Chang, C.L.; Yi, J. A Case of Chronic Gordonia otitidis Lung Infection Initially Regarded as Nontuberculous Mycobacterial Lung Disease. Ann. Clin. Microbiol. 2017, 20, 13. [Google Scholar] [CrossRef] [Green Version]
  51. Drancourt, M.; McNeil, M.M.; Brown, J.M.; Lasker, B.A.; Maurin, M.; Choux, M.; Raoult, D. Brain Abscess Due to Gordona terrae in an Immunocompromised Child: Case Report and Review of Infections Caused by G. terrae. Clin. Infect. Dis. 1994, 19, 258–262. [Google Scholar] [CrossRef] [PubMed]
  52. Blaschke, A.J.; Bender, J.; Byington, C.L.; Korgenski, K.; Daly, J.; Petti, C.A.; Pavia, A.T.; Ampofo, K. Gordonia Species: Emerging Pathogens in Pediatric Patients That Are Identified by 16S Ribosomal RNA Gene Sequencing. Clin. Infect. Dis. 2007, 45, 483–486. [Google Scholar] [CrossRef] [Green Version]
  53. Ramanan, P.; Deziel, P.J.; Wengenack, N.L. Gordonia Bacteremia. J. Clin. Microbiol. 2013, 51, 3443–3447. [Google Scholar] [CrossRef] [Green Version]
  54. Verma, P.; Brown, J.M.; Nunez, V.H.; Morey, R.E.; Steigerwalt, A.G.; Pellegrini, G.J.; Kessler, H.A. Native Valve Endocarditis Due to Gordonia polyisoprenivorans: Case Report and Review of Literature of Bloodstream Infections Caused by Gordonia Species. J. Clin. Microbiol. 2006, 44, 1905–1908. [Google Scholar] [CrossRef] [Green Version]
  55. Yoo, J.R.; Kim, M.; Lee, K.H.; Yoo, S.J.; Hyun, C.L.; Bae, J.; Heo, S.T.; Park, Y.G. A Fatal Infection due to Gordonia Terrae. J. Dermatol. Res. Ther. 2016, 2, 033. [Google Scholar] [CrossRef]
  56. Hou, C.; Yang, Y.; Li, Z. A Chinese patient with peritoneal dialysis-related peritonitis caused by Gordonia terrae: A case report. BMC Infect. Dis. 2017, 17, 179. [Google Scholar] [CrossRef] [Green Version]
  57. Gómez, C.G.; Casañ, C.; Antequera, P.; Candel, C.; Blázquez, R. Catheter-related bloodstream infection caused by Gordonia terrae in a bone-marrow transplant patient: Case report and review of the literature. JMM Case Rep. 2014, 1, e001032. [Google Scholar] [CrossRef]
  58. Kofteridis, D.P.; Valachis, A.; Scoulica, E.; Christidou, A.; Maraki, S.; Samonis, G. Hickman catheter-related bacteremia caused by Gordonia sputi in a patient with breast cancer. J. Infect. Dev. Ctries. 2011, 6, 188–191. [Google Scholar] [CrossRef] [Green Version]
  59. Gupta, M.; Prasad, D.; Khara, H.S.; Alcid, D. A rubber-degrading organism growing from a human body. Int. J. Infect. Dis. 2010, 14, e75–e76. [Google Scholar] [CrossRef] [Green Version]
  60. Arenskötter, M.; Bröker, D.; Steinbüchel, A. Biology of the Metabolically Diverse Genus Gordonia. Appl. Environ. Microbiol. 2004, 70, 3195–3204. [Google Scholar] [CrossRef] [Green Version]
  61. Raghuram, A. Gordonia Catheter-related Bacteremia and Native Valve Endocarditis Treated with Ceftriaxone and Oral Ciprofloxacin—A Case Report and Review of the Literature. Infect. Non Infect. Dis. 2015, 1, 1–3. [Google Scholar] [CrossRef]
  62. Werno, A.M.; Anderson, T.P.; Chambers, S.T.; Laird, H.M.; Murdoch, D.R. Recurrent Breast Abscess Caused by Gordonia bronchialis in an Immunocompetent Patient. J. Clin. Microbiol. 2005, 43, 3009–3010. [Google Scholar] [CrossRef] [Green Version]
  63. Brust, J.C.M.; Whittier, S.; Scully, B.E.; McGregor, C.C.; Yin, M.T. Five cases of bacteraemia due to Gordonia species. J. Med. Microbiol. 2009, 58, 1376–1378. [Google Scholar] [CrossRef]
  64. Kummer, C.; Schumann, P.; Stackebrandt, E. Gordonia alkanivorans sp. nov.; isolated from tar-contaminated soil. Int. J. Syst. Evol. Microbiol. 1999, 49, 1513–1522. [Google Scholar] [CrossRef]
  65. Akrami, K.; Coletta, J.; Mehta, S.; Fierer, J. Gordonia sternal wound infection treated with ceftaroline: Case report and literature review. JMM Case Rep. 2017, 4, e005113. [Google Scholar] [CrossRef] [Green Version]
  66. Franczuk, M.; Klatt, M.; Filipczak, D.; Zabost, A.; Parniewski, P.; Kuthan, R.; Jakubowska, L.; Augustynowicz-Kopeć, E. From NTM (Nontuberculous mycobacterium) to Gordonia bronchialis—A Diagnostic Challenge in the COPD Patient. Diagnostics 2022, 12, 307. [Google Scholar] [CrossRef]
  67. Jannat-Khah, D.P.; Halsey, E.S.; Lasker, B.A.; Steigerwalt, A.G.; Hinrikson, H.P.; Brown, J.M. Gordonia araii Infection Associated with an Orthopedic Device and Review of the Literature on Medical Device-Associated Gordonia Infections. J. Clin. Microbiol. 2009, 47, 499–502. [Google Scholar] [CrossRef] [Green Version]
  68. Kobayashi, T.; Otake, S.; Mori, T.; Hasegawa, D.; Kosaka, Y.; Ohkusu, K.; Kasai, M. A pediatric case of Gordonia otitidis bacteremia detected by long-term blood culture. J. Infect. Chemother. 2022, 28, 1427–1429. [Google Scholar] [CrossRef]
  69. Blanc, V.; Dalle, M.; Markarian, A.; Debunne, M.V.; Duplay, E.; Rodriguez-Nava, V.; Boiron, P. Gordonia terrae: A Difficult-To-Diagnose Emerging Pathogen? J. Clin. Microbiol. 2007, 45, 1076–1077. [Google Scholar] [CrossRef] [Green Version]
  70. Adams, T.; Brye, K.; Savin, M.; Lee, J.A.; Gbur, E. Microbial Carbon Substrate Utilization Differences among High- and Average-Yield Soybean Areas. Agriculture 2017, 7, 48. [Google Scholar] [CrossRef] [Green Version]
  71. Ercibengoa Arana, M.; Alonso, M.; Idigoras, P.; Vicente, D.; Marimón, J.M. Matrix-assisted laser desorption ionization-time of flight mass spectrometry (MALDI-TOF) score algorithm for identification of Gordonia species. AMB Express 2018, 8, 121. [Google Scholar] [CrossRef] [PubMed]
  72. Alcolea-Medina, A.; Fernandez, M.T.C.; Montiel, N.; García, M.P.L.; Sevilla, C.D.; North, N.; Lirola, M.J.M.; Wilks, M. An improved simple method for the identification of Mycobacteria by MALDI-TOF MS (Matrix-Assisted Laser Desorption- Ionization mass spectrometry). Sci. Rep. 2019, 9, 20216. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  73. Randall, L.P.; Lemma, F.; Koylass, M.; Rogers, J.; Ayling, R.D.; Worth, D.; Klita, M.; Steventon, A.; Line, K.; Wragg, P.; et al. Evaluation of MALDI-ToF as a method for the identification of bacteria in the veterinary diagnostic laboratory. Res. Vet. Sci. 2015, 101, 42–49. [Google Scholar] [CrossRef] [PubMed]
  74. Rodriguez-Lozano, J.; Pérez-Llantada, E.; Agüero, J.; Rodríguez-Fernández, A.; Ruiz de Alegria, C.; Martinez-Martinez, L.; Calvo, J. Sternal wound infection caused by Gordonia bronchialis: Identification by MALDI-TOF MS. JMM Case Rep. 2016, 3, e005067. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  75. Barberis, C.; Almuzara, M.; Join-Lambert, O.; Ramírez, M.S.; Famiglietti, A.; Vay, C. Comparison of the Bruker MALDI-TOF Mass Spectrometry System and Conventional Phenotypic Methods for Identification of Gram-Positive Rods. PLoS ONE 2014, 9, e106303. [Google Scholar] [CrossRef] [Green Version]
  76. Mormeneo Bayo, S.; Palacián Ruíz, M.P.; Asin Samper, U.; Millán Lou, M.I.; Pascual Catalán, A.; Villuendas Usón, M.C. Pacemaker-induced endocarditis by Gordonia bronchialis. Enferm. Infecc. Y Microbiol. Clínica 2022, 40, 255–257. [Google Scholar] [CrossRef]
  77. Chang, J.-H.; Ji, M.; Hong, H.-L.; Choi, S.-H.; Kim, Y.-S.; Chung, C.-H.; Sung, H.; Kim, M.-N. Sternal Osteomyelitis Caused by Gordonia bronchialis after Open-Heart Surgery. Infect. Chemother. 2014, 46, 110. [Google Scholar] [CrossRef] [Green Version]
  78. Martín, D.; Barrios, A.; Domingo, D.; Sánchez, P.; Sánchez, M.; Ruiz-Dassy, A.; Miqueleiz, A.; Sanz, J. Cerebrospinal fluid shunt-associated meningitis caused by Gordonia sputi: Case report and review of the literature. Le Infez. Med. 2017, 25, 174–178. [Google Scholar]
  79. Lam, J.Y.W.; Wu, A.K.L.; Leung, W.-S.; Cheung, I.; Tsang, C.-C.; Chen, J.H.K.; Chan, J.F.W.; Tse, C.W.S.; Lee, R.A.; Lau, S.K.P.; et al. Gordonia Species as Emerging Causes of Continuous-Ambulatory-Peritoneal-Dialysis-Related Peritonitis Identified by 16S rRNA and secA1 Gene Sequencing and Matrix-Assisted Laser Desorption Ionization–Time of Flight Mass Spectrometry (MALDI-TOF MS). J. Clin. Microbiol. 2015, 53, 671–676. [Google Scholar] [CrossRef] [Green Version]
  80. Sukackiene, D.; Rimsevicius, L.; Kiveryte, S.; Marcinkeviciene, K.; Bratchikov, M.; Zokaityte, D.; Tyla, R.; Laucyte-Cibulskiene, A.; Miglinas, M. A case of successfully treated relapsing peritoneal dialysis-associated peritonitis caused by Gordonia bronchialis in a farmer. Néphrologie Thérapeutique 2018, 14, 109–111. [Google Scholar] [CrossRef]
  81. Hsueh, P.-R.; Lee, T.-F.; Du, S.-H.; Teng, S.-H.; Liao, C.-H.; Sheng, W.-H.; Teng, L.-J. Bruker Biotyper Matrix-Assisted Laser Desorption Ionization–Time of Flight Mass Spectrometry System for Identification of Nocardia, Rhodococcus, Kocuria, Gordonia, Tsukamurella, and Listeria Species. J. Clin. Microbiol. 2014, 52, 2371–2379. [Google Scholar] [CrossRef] [Green Version]
  82. Sowani, H.; Kulkarni, M.; Zinjarde, S.; Javdekar, V. Gordonia and Related Genera as Opportunistic Human Pathogens Causing Infections of Skin, Soft Tissues, and Bones. In The Microbiology of Skin, Soft Tissue, Bone and Joint Infections; Elsevier: Amsterdam, The Netherlands, 2017; pp. 105–121. [Google Scholar] [CrossRef]
  83. Alshamaony, L.; Goodfellow, M.; Minnikin, D.E. Free Mycolic Acids as Criteria in the Classification of Nocardia and the “rhodochrous” Complex. J. Gen. Microbiol. 1976, 92, 188–199. [Google Scholar] [CrossRef] [Green Version]
  84. Collins, M.D.; Goodfellow, M.; Minnikin, D.E. A Survey of the Structures of Mycolic Acids in Corynebacterium and Related Taxa. Microbiology 1982, 128, 129–149. [Google Scholar] [CrossRef] [Green Version]
  85. Butler, W.R.; Jost, K.C.; Kilburn, J.O. Identification of mycobacteria by high-performance liquid chromatography. J. Clin. Microbiol. 1991, 29, 2468–2472. [Google Scholar] [CrossRef] [Green Version]
  86. Gordon, R.E.; Mihm, J.M. A Comparison of Nocardia asteroides and Nocardia brasiliensis. J. Gen. Microbiol. 1959, 20, 129–135. [Google Scholar] [CrossRef] [Green Version]
  87. Gordon, R.E.; Mihm, J.M. The Type Species of the Genus Nocardia. J. Gen. Microbiol. 1962, 27, 1–10. [Google Scholar] [CrossRef] [Green Version]
  88. Becker, B.; Lechevalier, M.P.; Gordon, R.E.; Lechevalier, H.A. Rapid Differentiation Between Nocardia and Streptomyces by Paper Chromatography of Whole-Cell Hydrolysates. Appl. Microbiol. 1964, 12, 421–423. [Google Scholar] [CrossRef]
  89. Lechevalier, M.P. Identification of aerobic actinomycetes of clinical importance. J. Lab. Clin. Med. 1968, 71, 934–944. [Google Scholar]
  90. Aoyama, K.; Kang, Y.; Yazawa, K.; Gonoi, T.; Kamei, K.; Mikami, Y. Characterization of Clinical Isolates of Gordonia Species in Japanese Clinical Samples during 1998–2008. Mycopathologia 2009, 168, 175–183. [Google Scholar] [CrossRef]
  91. Lechevalier, M.P.; Lechevalier, H. Chemical composition as a criterion in the classification of aerobic actinomycetes. Int. J. Syst. Bacteriol. 1970, 20, 435–443. [Google Scholar] [CrossRef] [Green Version]
  92. Jacques, M.-A.; Durand, K.; Orgeur, G.; Balidas, S.; Fricot, C.; Bonneau, S.; Quillévéré, A.; Audusseau, C.; Olivier, V.; Grimault, V.; et al. Phylogenetic Analysis and Polyphasic Characterization of Clavibacter michiganensis Strains Isolated from Tomato Seeds Reveal that Nonpathogenic Strains Are Distinct from C. michiganensis subsp. michiganensis. Appl. Environ. Microbiol. 2012, 78, 8388–8402. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  93. Ratnikova, M.S.; Titok, M.A. Molecular Genetic Markers for Identification of Rhodococcus erythropolis and Rhodococcus qingshengii. Microbiology 2020, 89, 435–442. [Google Scholar] [CrossRef]
  94. Van de Peer, Y. A quantitative map of nucleotide substitution rates in bacterial rRNA. Nucleic Acids Res. 1996, 24, 3381–3391. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  95. Cole, J.R.; Wang, Q.; Fish, J.A.; Chai, B.; McGarrell, D.M.; Sun, Y.; Brown, C.T.; Porras-Alfaro, A.; Kuske, C.R.; Tiedje, J.M. Ribosomal Database Project: Data and tools for high throughput rRNA analysis. Nucleic Acids Res. 2014, 42, D633–D642. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  96. McDonald, D.; Price, M.N.; Goodrich, J.; Nawrocki, E.P.; DeSantis, T.Z.; Probst, A.; Andersen, G.L.; Knight, R.; Hugenholtz, P. An improved Greengenes taxonomy with explicit ranks for ecological and evolutionary analyses of bacteria and archaea. ISME J. 2012, 6, 610–618. [Google Scholar] [CrossRef]
  97. Quast, C.; Pruesse, E.; Yilmaz, P.; Gerken, J.; Schweer, T.; Yarza, P.; Peplies, J.; Glöckner, F.O. The SILVA ribosomal RNA gene database project: Improved data processing and web-based tools. Nucleic Acids Res. 2012, 41, D590–D596. [Google Scholar] [CrossRef]
  98. Yoon, S.-H.; Ha, S.-M.; Kwon, S.; Lim, J.; Kim, Y.; Seo, H.; Chun, J. Introducing EzBioCloud: A taxonomically united database of 16S rRNA gene sequences and whole-genome assemblies. Int. J. Syst. Evol. Microbiol. 2017, 67, 1613–1617. [Google Scholar] [CrossRef]
  99. Wang, B.; Cui, Z.; Yu, S.; Sun, D.; Zhang, W.; Jin, X.; Cheng, X.; Chen, Y. Rapid detection of Gordonia aichiensis by metagenomic next-generation sequencing in a patient with peritoneal dialysis-associated peritonitis. Perit. Dial. Int. J. Int. Soc. Perit. Dial. 2022, 42, 542–545. [Google Scholar] [CrossRef]
  100. Lesens, O. Bacteremia and Endocarditis Caused by a Gordonia Species in a Patient with a Central Venous Catheter. Emerg. Infect. Dis. 2000, 6, 382–385. [Google Scholar] [CrossRef] [Green Version]
  101. Wright, S.N.; Gerry, J.S.; Busowski, M.T.; Klochko, A.Y.; McNulty, S.G.; Brown, S.A.; Sieger, B.E.; Michaels, P.K.; Wallace, M.R. Gordonia bronchialis Sternal Wound Infection in 3 Patients following Open Heart Surgery: Intraoperative Transmission from a Healthcare Worker. Infect. Control Hosp. Epidemiol. 2012, 33, 1238–1241. [Google Scholar] [CrossRef]
  102. Shen, F.-T.; Young, C.-C. Rapid detection and identification of the metabolically diverse genus Gordonia by 16S rRNA-gene-targeted genus-specific primers. FEMS Microbiol. Lett. 2005, 250, 221–227. [Google Scholar] [CrossRef] [Green Version]
  103. Lai, C.C.; Wang, C.Y.; Liu, C.Y.; Tan, C.K.; Lin, S.H.; Liao, C.H.; Chou, C.H.; Huang, Y.T.; Lin, H.I.; Hsueh, P.R. Infections Caused by Gordonia Species at a Medical Center in Taiwan, 1997 to 2008. Clin. Microbiol. Infect. 2009, 16, 1448–1453. [Google Scholar] [CrossRef]
  104. Neilan, B.A.; Jacobs, D.; Therese, D.D.; Blackall, L.L.; Hawkins, P.R.; Cox, P.T.; Goodman, A.E. rRNA Sequences and Evolutionary Relationships among Toxic and Nontoxic Cyanobacteria of the Genus Microcystis. Int. J. Syst. Bacteriol. 1997, 47, 693–697. [Google Scholar] [CrossRef]
  105. Negishi, T.; Matsumoto, T.; Saito, S.; Kasuga, E.; Horiuchi, K.; Natori, T.; Takehara, K.; Sugano, M.; Honda, T. Catheter-Related Bacteremia Due to Gordonia sputi in a Patient with Acute Lymphocytic Leukemia: A Case Report. Jpn. J. Infect. Dis. 2016, 69, 342–343. [Google Scholar] [CrossRef] [Green Version]
  106. Bartolomé-Álvarez, J.; Sáez-Nieto, J.A.; Escudero-Jiménez, A.; Barba-Rodríguez, N.; Galán-Ros, J.; Carrasco, G.; Muñoz-Izquierdo, M.P. Cutaneous abscess due to Gordonia bronchialis: Case report and literature review. Rev. Esp. De Quimioter. Publ. Of. De La Soc. Esp. De Quimioter. 2016, 29, 170–173. [Google Scholar]
  107. Weisburg, W.G.; Barns, S.M.; Pelletier, D.A.; Lane, D.J. 16S ribosomal DNA amplification for phylogenetic study. J. Bacteriol. 1991, 173, 697–703. [Google Scholar] [CrossRef] [Green Version]
  108. Godon, J.J.; Zumstein, E.; Dabert, P.; Habouzit, F.; Moletta, R. Molecular microbial diversity of an anaerobic digestor as determined by small-subunit rDNA sequence analysis. Appl. Environ. Microbiol. 1997, 63, 2802–2813. [Google Scholar] [CrossRef] [Green Version]
  109. Pinto, A.J.; Raskin, L. PCR Biases Distort Bacterial and Archaeal Community Structure in Pyrosequencing Datasets. PLoS ONE 2012, 7, e43093. [Google Scholar] [CrossRef] [Green Version]
  110. Sun, D.-L.; Jiang, X.; Wu, Q.L.; Zhou, N.-Y. Intragenomic Heterogeneity of 16S rRNA Genes Causes Overestimation of Prokaryotic Diversity. Appl. Environ. Microbiol. 2013, 79, 5962–5969. [Google Scholar] [CrossRef] [Green Version]
  111. Johnson, J.S.; Spakowicz, D.J.; Hong, B.-Y.; Petersen, L.M.; Demkowicz, P.; Chen, L.; Leopold, S.R.; Hanson, B.M.; Agresta, H.O.; Gerstein, M.; et al. Evaluation of 16S rRNA gene sequencing for species and strain-level microbiome analysis. Nat. Commun. 2019, 10, 5029. [Google Scholar] [CrossRef] [Green Version]
  112. Eren, A.M.; Maignien, L.; Sul, W.J.; Murphy, L.G.; Grim, S.L.; Morrison, H.G.; Sogin, M.L. Oligotyping: Differentiating between closely related microbial taxa using 16S rRNA gene data. Methods Ecol. Evol. 2013, 4, 1111–1119. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  113. Peeters, K.; Willems, A. The gyrB gene is a useful phylogenetic marker for exploring the diversity of Flavobacterium strains isolated from terrestrial and aquatic habitats in Antarctica. FEMS Microbiol. Lett. 2011, 321, 130–140. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  114. Kang, Y.; Takeda, K.; Yazawa, K.; Mikami, Y. Phylogenetic Studies of Gordonia Species Based on gyrB and secA1 Gene Analyses. Mycopathologia 2009, 167, 95–105. [Google Scholar] [CrossRef] [PubMed]
  115. Marchese, A.; Debbia, E.A. The role of gyrA, gyrB, and dnaA functions in bacterial conjugation. Ann. Microbiol. 2016, 66, 223–228. [Google Scholar] [CrossRef]
  116. Hurtle, W.; Bode, E.; Kulesh, D.A.; Kaplan, R.S.; Garrison, J.; Bridge, D.; House, M.; Frye, M.S.; Loveless, B.; Norwood, D. Detection of the Bacillus anthracis gyrA Gene by Using a Minor Groove Binder Probe. J. Clin. Microbiol. 2004, 42, 179–185. [Google Scholar] [CrossRef] [Green Version]
  117. Chun, J. Phylogenetic analysis of Bacillus subtilis and related taxa based on partial gyrA gene sequences. Antonie Van Leeuwenhoek 2000, 78, 123–127. [Google Scholar] [CrossRef]
  118. Shen, F.-T.; Lu, H.-L.; Lin, J.-L.; Huang, W.-S.; Arun, A.B.; Young, C.-C. Phylogenetic analysis of members of the metabolically diverse genus Gordonia based on proteins encoding the gyrB gene. Res. Microbiol. 2006, 157, 367–375. [Google Scholar] [CrossRef]
  119. Delegan, Y.A.; Vetrova, A.A.; Akimov, V.N.; Titok, M.A.; Filonov, A.E.; Boronin, A.M. Thermotolerant oil-degrading bacteria isolated from soil and water of geographically distant regions. Appl. Biochem. Microbiol. 2016, 52, 389–396. [Google Scholar] [CrossRef]
  120. Yamamoto, S.; Harayama, S. PCR amplification and direct sequencing of gyrB genes with universal primers and their application to the detection and taxonomic analysis of Pseudomonas putida strains. Appl. Environ. Microbiol. 1995, 61, 1104–1109. [Google Scholar] [CrossRef] [Green Version]
  121. Johnson, J.A.; Onderdonk, A.B.; Cosimi, L.A.; Yawetz, S.; Lasker, B.A.; Bolcen, S.J.; Brown, J.M.; Marty, F.M. Gordonia bronchialis Bacteremia and Pleural Infection: Case Report and Review of the Literature. J. Clin. Microbiol. 2011, 49, 1662–1666. [Google Scholar] [CrossRef] [Green Version]
  122. Ishikawa, J.; Yamashita, A.; Mikami, Y.; Hoshino, Y.; Kurita, H.; Hotta, K.; Shiba, T.; Hattori, M. The complete genomic sequence of Nocardia farcinica IFM 10152. Proc. Natl. Acad. Sci. 2004, 101, 14925–14930. [Google Scholar] [CrossRef] [Green Version]
  123. Takeda, K.; Kang, Y.; Yazawa, K.; Gonoi, T.; Mikami, Y. Phylogenetic studies of Nocardia species based on gyrB gene analyses. J. Med. Microbiol. 2010, 59, 165–171. [Google Scholar] [CrossRef] [Green Version]
  124. Lasker, B.A.; Moser, B.D.; Brown, J. Gordonia, in Molecular Detection of Human Bacterial Pathogens, 1st ed.; Section I Actinobacteria; CRC Press: Boca Raton, FL, USA, 2011; ISBN 9781439812389. [Google Scholar]
  125. Chaudhary, A.S.; Chen, W.; Jin, J.; Tai, P.C.; Wang, B. SecA: A potential antimicrobial target. Future Med. Chem. 2015, 7, 989–1007. [Google Scholar] [CrossRef]
  126. Lill, R.; Dowhan, W.; Wickner, W. The ATPase activity of secA is regulated by acidic phospholipids, secY, and the leader and mature domains of precursor proteins. Cell 1990, 60, 271–280. [Google Scholar] [CrossRef]
  127. Conville, P.S.; Zelazny, A.M.; Witebsky, F.G. Analysis of secA1 Gene Sequences for Identification of Nocardia Species. J. Clin. Microbiol. 2006, 44, 2760–2766. [Google Scholar] [CrossRef] [Green Version]
  128. Zelazny, A.M.; Calhoun, L.B.; Li, L.; Shea, Y.R.; Fischer, S.H. Identification of Mycobacterium Species by secA1 Sequences. J. Clin. Microbiol. 2005, 43, 1051–1058. [Google Scholar] [CrossRef] [Green Version]
  129. Steingrube, V.A.; Gibson, J.L.; Brown, B.A.; Zhang, Y.; Wilson, R.W.; Rajagopalan, M.; Wallace, R.J. PCR amplification and restriction endonuclease analysis of a 65-kilodalton heat shock protein gene sequence for taxonomic separation of rapidly growing mycobacteria. J. Clin. Microbiol. 1995, 33, 149–153. [Google Scholar] [CrossRef] [Green Version]
  130. Telenti, A.; Marchesi, F.; Balz, M.; Bally, F.; Böttger, E.C.; Bodmer, T. Rapid identification of mycobacteria to the species level by polymerase chain reaction and restriction enzyme analysis. J. Clin. Microbiol. 1993, 31, 175–178. [Google Scholar] [CrossRef] [Green Version]
  131. Roth, A.; Reischl, U.; Streubel, A.; Naumann, L.; Kroppenstedt, R.M.; Habicht, M.; Fischer, M.; Mauch, H. Novel Diagnostic Algorithm for Identification of Mycobacteria Using Genus-Specific Amplification of the 16S-23S rRNA Gene Spacer and Restriction Endonucleases. J. Clin. Microbiol. 2000, 38, 1094–1104. [Google Scholar] [CrossRef] [Green Version]
  132. Senna, S.G.; Battilana, J.; Costa, J.C.; Silva, M.G.; Duarte, R.S.; Fonseca, L.S.; Suffys, P.N.; Bogo, M.R. Sequencing of hsp65 Gene for Identification of Mycobacterium Species Isolated from Environmental and Clinical Sources in Rio de Janeiro, Brazil. J. Clin. Microbiol. 2008, 46, 3822–3825. [Google Scholar] [CrossRef] [Green Version]
  133. Sheng, W.-H.; Huang, Y.-T.; Chang, S.-C.; Hsueh, P.-R. Brain Abscess Caused by Tsukamurella tyrosinosolvens in an Immunocompetent Patient. J. Clin. Microbiol. 2009, 47, 1602–1604. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  134. Arenskötter, M.; Baumeister, D.; Berekaa, M.M.; Pötter, G.; Kroppenstedt, R.M.; Linos, A.; Steinbüchel, A. Taxonomic characterization of two rubber degrading bacteria belonging to the species Gordonia polyisoprenivorans and analysis of hyper variable regions of 16S rDNA sequences. FEMS Microbiol. Lett. 2001, 205, 277–282. [Google Scholar] [CrossRef] [PubMed]
  135. Kempf, V.A.J.; Schmalzing, M.; Yassin, A.F.; Schaal, K.P.; Baumeister, D.; Arenskötter, M.; Steinbuchel, A.; Autenrieth, I.B. Gordonia polyisoprenivorans Septicemia in a Bone Marrow Transplant Patient. Eur. J. Clin. Microbiol. Infect. Dis. 2004, 23, 226–228. [Google Scholar] [CrossRef] [PubMed]
  136. Moser, B.D.; Pellegrini, G.J.; Lasker, B.A.; Brown, J.M. Pattern of Antimicrobial Susceptibility Obtained from Blood Isolates of a Rare but Emerging Human Pathogen, Gordonia polyisoprenivorans. Antimicrob. Agents Chemother. 2012, 56, 4991–4993. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  137. Meier-Kolthoff, J.P.; Auch, A.F.; Klenk, H.-P.; Göker, M. Genome sequence-based species delimitation with confidence intervals and improved distance functions. BMC Bioinform. 2013, 14, 60. [Google Scholar] [CrossRef] [Green Version]
  138. Moore, W.E.C.; Stackebrandt, E.; Kandler, O.; Colwell, R.R.; Krichevsky, M.I.; Truper, H.G.; Murray, R.G.E.; Wayne, L.G.; Grimont, P.A.D.; Brenner, D.J.; et al. Report of the Ad Hoc Committee on Reconciliation of Approaches to Bacterial Systematics. Int. J. Syst. Evol. Microbiol. 1987, 37, 463–464. [Google Scholar] [CrossRef] [Green Version]
  139. Stackebrandt, E.; Goebel, B.M. Taxonomic Note: A Place for DNA-DNA Reassociation and 16S rRNA Sequence Analysis in the Present Species Definition in Bacteriology. Int. J. Syst. Evol. Microbiol. 1994, 44, 846–849. [Google Scholar] [CrossRef] [Green Version]
  140. Koenigsaecker, T.M.; Eisen, J.A.; Coil, D.A. Draft Genome Sequence of Gordonia sp. Strain UCD-TK1 (Phylum Actinobacteria). Genome Announc. 2016, 4, e01121-16. [Google Scholar] [CrossRef] [Green Version]
  141. Tritt, A.; Eisen, J.A.; Facciotti, M.T.; Darling, A.E. An Integrated Pipeline for de Novo Assembly of Microbial Genomes. PLoS ONE 2012, 7, e42304. [Google Scholar] [CrossRef] [Green Version]
  142. Gulvik, C.A.; Batra, D.; Rowe, L.A.; Sheth, M.; Nobles, S.; Lee, J.S.; McQuiston, J.R.; Lasker, B.A. Complete and Circularized Bacterial Genome Sequence of Gordonia sp. Strain X0973. Microbiol. Resour. Announc. 2021, 10, e01479-20. [Google Scholar] [CrossRef]
  143. Ahrholdt, J. Gordonia parafnivorans–ein seltener Mastitiserreger bei Rindern (Gordonia parafnivorans: An uncommon agent of bovine mastitis). Prakt. Tierarzt 2020, 101, 882–888. [Google Scholar] [CrossRef]
  144. Valkó, A. Corynebacterinae Alrendbe Tartozó TőgygyulladáS-kórokozó baktériumok Diagnosztikai Vizsgálatai (Identification of Mastitis Causing Bacteria in the Corynebacterinae Suborder). Szent István Egyetem Állatorvos-tudományi Kar, Budapest, Hungary. Thesis. 2014, p. 39. Available online: http://www.huveta.hu/handle/10832/1350 (accessed on 26 March 2021).
  145. Brown-Elliott, B.A.; Brown, J.M.; Conville, P.S.; Wallace, R.J. Clinical and Laboratory Features of the Nocardia spp. Based on Current Molecular Taxonomy. Clin. Microbiol. Rev. 2006, 19, 259–282. [Google Scholar] [CrossRef] [Green Version]
  146. Buchman, A.L.; McNeil, M.M.; Brown, J.M.; Lasker, B.A.; Amentn, M.E. Central Venous Catheter Sepsis Caused by Unusual Gordona (Rhodococcus) Species: Identification with a Digoxigenin-Labeled rDNA Probe. Clin. Infect. Dis. 1992, 15, 694–697. [Google Scholar] [CrossRef]
  147. Pham, A.S.; De, I.; Rolston, K.V.; Tarrand, J.J.; Han, X.Y. Catheter-Related Bacteremia Caused by the Nocardioform Actinomycete Gordonia terrae. Clin. Infect. Dis. 2003, 36, 524–527. [Google Scholar] [CrossRef]
Table
Table 1. Information concerning Gordonia species whose type strains were newly isolated from clinical samples.
Table 1. Information concerning Gordonia species whose type strains were newly isolated from clinical samples.
SpeciesType of SampleDiseaseIdentification ApproachReference
Gordonia otitidisear dischargeexternal otitismycolic acid profile, compound utilization patterns, 16S rRNA gene sequencing[26]
Gordonia araiisputumbacterial pneumoniaTLC, HPLC, 16S rRNA gene sequencing, DNA–DNA hybridization[27]
Gordonia effusasputumkidney dysfunctionTLC, HPLC, 16S rRNA gene sequencing, DNA–DNA hybridization[27]
Gordonia iteranssputumbacterial pneumoniaTLC, mycolic acid profile, 16S rRNA gene sequencing, DNA–DNA hybridization[28]
Gordonia aichiensis (previously, Rhodococcus aichiensis)sputumpulmonary diseasemycolic acid profile, 16S rRNA sequencing[29]
Gordonia bronchialissputumcavitary pulmonary tuberculosis and/or bronchiectasismycolic acid profile, compound utilization patterns[30]
Gordonia sputi (previously, Rhodococcus sputi)sputumpulmonary diseasemycolic acid profile, compound utilization patterns[31]
Gordonia jinhuaensispharmaceutical wastewater-HPLC, 16S rRNA gene sequencing, compound utilization patterns[32]
Gordonia croceadrainage stripswound infection after pacemaker implantationMALDI TOF MS, 16S rRNA gene sequencing[33]
Gordonia hongkongensis(1) blood culture, (2) the peritoneal dialysis effluent(1) continuous ambulatory peritoneal dialysis (CAPD)-related peritonitis, (2) bacteraemiaHPLC, 16S rRNA, gyrB, secA genes sequencing, DNA–DNA hybridization[34]
Abbreviations: TLC—thin-layer chromatography; HPLC—high-performance liquid chromatography.
Table
Table 2. Gordonia species, the type strains of which were initially isolated from environmental samples. Some strains of these species are human or veterinary pathogens.
Table 2. Gordonia species, the type strains of which were initially isolated from environmental samples. Some strains of these species are human or veterinary pathogens.
SpeciesDiseaseReference to an Article with an Example of a Pathogenic StrainIsolation Source of the Type StrainReference to an Article with Type Strain Isolation
Gordonia amicaliscutaneous infection after a traumatic injury[35]soil contaminated with thiophenes[10]
“Gordonia jacobaea”prosthetic joint septic arthritis[36]soil[37]
Gordonia paraffinivoranscow mastitis[38]oil-producing well of Daqing oilfield[39]
Gordonia polyisoprenivoranscatheter-related bacteremia[40]automobile tyre[41]
Gordonia rubripertinctalung infection[42]soil[43]
Gordonia sinesedisLymphadenitis[44]soil[45]
Gordonia terraeacute cholecystitis[46]soil[47]
Gordonia westfalicamycetoma of the foot[48]foul water taken from the inside of a deteriorated automobile tyre[14]
Table
Table 3. Examples of matching the identification of Gordonia strains using the MALDI method and genetic methods.
Table 3. Examples of matching the identification of Gordonia strains using the MALDI method and genetic methods.
Genus/Species Determined by the MALDIBruker Biotyper VersionNumber of Identification RepetitionsScoresThe Result of Identification by an Additional ApproachThe Approach Used for Additional IdentificationReference
G. bronchialisND21.68, 2.08G. bronchialis16S rRNA[76]
G. bronchialisND11.83G. bronchialisgyrB[65]
G. rubripertincta3.011.764G. polyisoprenivorans16S rRNA, gyrB[40]
G. bronchialisND11.808G. bronchialis16S rRNA, hsp65[77]
G. sputiND21.65, 1.57G. sputi16S rRNA[78]
G. bronchialisND2-G. bronchialis16S rRNA[66] *
G. sputi3.112.039G. sputi16S rRNA, secA1[79]
G. sputi12.026G. sputi16S rRNA, secA1
G. bronchialis11.743G. bronchialis16S rRNA, secA1
Gordonia sp.11.550G. lacunae/G. terrae/new species16S rRNA, secA1
G. rubripertinctaND1-G. bronchialis16S rRNA[80]
G. rubripertincta4.11(for 27 samples) 1.723–2.319G. paraffinovoransWGS[38]
G. rubropertinctaND11.702G. terrae16S rRNA[56]
* The modified protocol was used because the standard one gave no result. ND—no data.
Table
Table 4. Primers used for amplification of genes/fragments of 16S rRNA genes in the identification of Gordonia.
Table 4. Primers used for amplification of genes/fragments of 16S rRNA genes in the identification of Gordonia.
№Primer NamePrimer SequenceSpecies IdentifiedReference
1P8-275′-AGA GTT TGA TCC TGG CTC AG-3′universal[52,63,100]
P1392-13725′-AAG GCC CGG GAA CGT ATT CAC-3′
216S-F5′-AGA GTT TGA TCC TGG CTC AG-3′G. bronchialis[76]
16S-R5′-ACG GCT ACC TTG TTA CGA CTT-3′
3fD15′-CCG AAT TCG TCG ACA ACA GAG TTT GAT CCT GGC TCA G-3′G. polyisoprenivorans[54]
rD15′-CCC GGG ATC CAA GCT TAA GGA GGT GAT CCA GCC-3′
427FLP5′-AGA GTT TGA TCM TGG CTC AG-3′G. terrae[55]
1492RPL5′-GGT TAC CTT GTT ACG ACT T-3′
5-5′-TGG AGA GTT TGA TCC TGG CTC AG-3′G. bronchialis[101]
-5′-TAC CGC GGC TGC TGG CAC-3′
6BACT5′-CAG GCC TAA CAC ATG CAA GTC-3′G. sputi[58]
UNI5′-GAC GGG CGG TGT GTA CAA-3′
7G268F5′-CGA CCT GAG AGG GTG ATC G-3′G. sputi, G. bronchialis, G. terrae/lacumae[79,102]
G1096R5′-ATA ACC CGC TGG CAA TAC AG-3′
88FLP5′-AGA GTT TGA TCC TGG CTC AG-3′G. terrae, G. sputi[103]
1492RPL5′-GGT TAC CTT GTT ACG ACT T-3′
95F5′-TTG GAG AGT TTG ATC CTG GCT C-3′G. terrae, G. otitidis, G. bronchialis[52]
1194R5′-ACG TCA TCC CCA CCT TCC TC-3′
1027FI5′-AGA GTT TGA TCC TGG CTC AG-3′G. sputi[104,105]
1494Rc5′-TAC GGC TAC CTT GTT ACG AC-3′
11fD15′-CCG AAT TCG TCG ACA ACA GAG TTT GAT CCT GGC TCA G-3′G. bronchialis[106,107]
rP25′-CCC GGG ATC CAA GCT TAC GGC TAC CTT GTT ACG ACT T-3′
1227F5′-GAG TTT GAT CCT GGC TCA G-3′G. terrae[56]
1492R5′-AAG GAG GTG ATC CAG CCG CA-3′
135F5′-TGG AGA GTT TGA TCC TGG CTA G-3′G. sputi, G. otitidis, G. bronchialis[71]
1193R5′-ACG TCA TCC CCG CTT CCT T-3′
14w0015′-AGA GTT TGA TCM TGG CTC-3′G. bronchialis[80,108]
w0025′-GNT ACC TTG TTA CGA CTT-3′
Table
Table 5. Sequences of primers used for amplification of gyrB genes/fragments in Gordonia strains.
Table 5. Sequences of primers used for amplification of gyrB genes/fragments in Gordonia strains.
Primer NamePrimer SequenceSpeciesReference
GYRB15′-ATG CAN CAR YTN CAY GCN GGN-3′universal[118]
GYRB25′-SAY GAT CTT GTK RTA SCG MAA YTT-3′
UP-15′-GAA GTC ATC ATG ACC GTT CTG CAY GCN GGN GGN AAR TTY GA-3′universal[120]
UP-25′-AGC AGG GTA CGG ATG TGC GAG CCR TCN ACR TCN GCR TCN GTC AT-3′
UP1F5′-GAG GTC GTC ATG ACC CAG CTG CAY GCN GGN GGN AAR TTY GA-3′G. otitidis[50]
UP2r-modi5′-AGC AGC GTC GAG ATG TGC TGG CCR TCN ACR TCN GCR TCN GTC A-3′
Table
Table 6. Sequences of primers used for amplification of secA genes/fragments in Gordonia strains.
Table 6. Sequences of primers used for amplification of secA genes/fragments in Gordonia strains.
Primer NamePrimer SequenceReference
SecA1-f5′-GTA AAA CGA CGG CCA GGA CAG YGA GTG GAT GGG YCG SGT GCA CCG-3′[114]
SecA1-r5′-CAG GAA ACA GCT ATG ACG CGG ACG ATG TAG TCC TTG TC-3′
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Frantsuzova, E.; Bogun, A.; Vetrova, A.; Delegan, Y. Methods of Identifying Gordonia Strains in Clinical Samples. Pathogens 2022, 11, 1496. https://doi.org/10.3390/pathogens11121496

AMA Style

Frantsuzova E, Bogun A, Vetrova A, Delegan Y. Methods of Identifying Gordonia Strains in Clinical Samples. Pathogens. 2022; 11(12):1496. https://doi.org/10.3390/pathogens11121496

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Frantsuzova, Ekaterina, Alexander Bogun, Anna Vetrova, and Yanina Delegan. 2022. "Methods of Identifying Gordonia Strains in Clinical Samples" Pathogens 11, no. 12: 1496. https://doi.org/10.3390/pathogens11121496

APA Style

Frantsuzova, E., Bogun, A., Vetrova, A., & Delegan, Y. (2022). Methods of Identifying Gordonia Strains in Clinical Samples. Pathogens, 11(12), 1496. https://doi.org/10.3390/pathogens11121496

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