4c eyebrows

4c eyebrows DEFAULT

Leprosy in wild chimpanzees


Humans are considered as the main host for Mycobacterium leprae1, the aetiological agent of leprosy, but spillover has occurred to other mammals that are now maintenance hosts, such as nine-banded armadillos and red squirrels2,3. Although naturally acquired leprosy has also been described in captive nonhuman primates4,5,6,7, the exact origins of infection remain unclear. Here we describe leprosy-like lesions in two wild populations of western chimpanzees (Pan troglodytes verus) in Cantanhez National Park, Guinea-Bissau and Taï National Park, Côte d’Ivoire, West Africa. Longitudinal monitoring of both populations revealed the progression of disease symptoms compatible with advanced leprosy. Screening of faecal and necropsy samples confirmed the presence of M. leprae as the causative agent at each site and phylogenomic comparisons with other strains from humans and other animals show that the chimpanzee strains belong to different and rare genotypes (4N/O and 2F). These findings suggest that M. leprae may be circulating in more wild animals than suspected, either as a result of exposure to humans or other unknown environmental sources.


Leprosy is a neglected tropical disease caused by the bacterial pathogens M. leprae and the more recently discovered Mycobacteriumlepromatosis8,9. In humans, the disease presents as a continuum of clinical manifestations with skin and nerve lesions of increasing severity, from the mildest tuberculoid form (or paucibacillary) to the most severe lepromatous type (or multibacillary)10. Symptoms develop after a long incubation period ranging from several months to 30 years, averaging 5 years in humans. As a result of sensory loss, leprosy can lead to permanent damage and severe deformity11. Although leprosy prevalence has markedly decreased over recent decades, approximately 210,000 new human cases are still reported every year, of which 2.3% are located in West Africa12. Transmission is thought to occur primarily between individuals with prolonged and close contact via aerosolized nasal secretions and entry through nasal or respiratory mucosae, but the exact mechanism remains unclear13,14. The role of other routes, such as skin-to-skin contact, is unknown.

Leprosy-causing bacteria were once thought to be obligate human pathogens1. However, they can circulate in other animal hosts in the wild, such as nine-banded armadillos (Dasypusnovemcinctus) in the Americas and red squirrels (Sciurusvulgaris) in the UK2,3. Although initial infection was most probably incidental and of human origin, secondary animal hosts can subsequently represent a source of infection to humans15,16,17,18. In captivity, nonhuman primates, such as chimpanzees (Pantroglodytes)4, sooty mangabeys (Cercocebusatys)5,6 and cynomolgus macaques (Macacafascicularis)7, have been known to develop leprosy without any obvious infectious source. However, due to their captive status, it is unclear how they acquired M. leprae and whether these species can also contract leprosy in the wild.

Here, we report leprosy infections and their disease course in two wild populations of western chimpanzees (P. troglodytes verus) in Cantanhez National Park (CNP), Guinea-Bissau, and in Taï National Park (TNP), Côte d’Ivoire, using a combination of camera trap and veterinary monitoring (Extended Data Fig. 1a and Supplementary Notes 1 and 2). From analyses of faecal samples and postmortem tissues, we identified M. leprae as the causative agent of the lesions observed and determined the phylogenetic placement of the respective strains based on their complete genome sequences.

Chimpanzees at CNP are not habituated to human observers, precluding systematic behavioural observations. Longitudinal studies necessitate the use of camera traps, which we operated between 2015 and 2019. Of 624,194 data files (videos and photographs) obtained across 211 locations at CNP (Extended Data Fig. 1b, Extended Data Table 1 and Supplementary Table 1), 31,044 (5.0%) contained chimpanzees. The number of independent events (images separated by at least 60 min) totalled 4,336, and of these, 241 (5.6%) contained chimpanzees with severe leprosy-like lesions, including four clearly identifiable individuals (two adult females and two adult males) across three communities (Extended Data Fig. 2 and Supplementary Note 2). As with humans, paucibacillary cases in chimpanzees may be present but easily go undetected. Such minor manifestations of leprosy are not reported. All symptomatic chimpanzees showed hair loss and facial skin hypopigmentation, as well as plaques and nodules that covered different areas of their body (limbs, trunk and genitals), facial disfigurement and ulcerated and deformed hands (claw hand) and feet (Fig. 1a–c), consistent with a multibacillary form of the disease. Longitudinal observations showed progression of symptoms across time with certain manifestations similar to those described in humans (such as progressive deformation of the hands) (Extended Data Fig. 2 and Supplementary Videos 1–3). To confirm infection with M. leprae, we collected faecal samples and tested them with two nested polymerase chain reaction (PCR) assays targeting the M. leprae-specific repetitive element (RLEP) and 18 kDa antigen gene. One out of 208 DNA extracts from CNP was positive in both assays and a second was positive only in the more sensitive RLEP-PCR19 (Extended Data Table 2, Supplementary Table 2 and Supplementary Note 3). Microsatellite analyses of the two positive samples confirmed that they originated from two distinct female individuals (Supplementary Note 4 and Supplementary Tables 3 and 4). Our results suggest that M. leprae is the most likely cause of a leprosy-like syndrome in chimpanzees from CNP.

a–c, Clinical signs of leprosy in two adult female chimpanzees in CNP (images extracted from camera traps). a, Rita has large hypopigmented nodules covering the entire body; disfigurement of the face, ears, hands and feet (ulcerated lesions and swelling). b, Rita has extensive plaques covering all limbs, with hair loss. c, Brinkos has large hypopigmented nodules covering the entire face, with extreme disfigurement of the face and ears, and ulcerated plaques on the arms and the nipples. dg, Clinical signs of leprosy in an adult male chimpanzee, Woodstock, at TNP. d, Multiple hypopigmented nodules on the ears, brow ridges, eyelid margins, nostrils, lips and the area between the upper lip and the nose. e, Hypopigmentation and swelling of the hands with ulcerations and hair loss on the dorsal side of the joints. f, Claw hand with nail loss and abnormal overgrowth of fingernails. g, Scrotal reddening and ulceration with fresh blood.

Full size image

At TNP, chimpanzees are habituated to the presence of researchers and have been followed daily since 1979. In addition, necropsy samples have been collected from all dead individuals recovered since 2000. In June 2018, researchers first noticed leprosy-like lesions on Woodstock, an adult male chimpanzee from one of the three habituated communities (south) (Extended Data Fig. 1c). The initial small nodules on the ears, lips and under the eye became more prominent and were followed by nodules on the eyebrows, eyelids, nostrils, ears, lips and face. The skin on facial nodules, hands, feet and testicles became hypopigmented and the loss and abnormal growth of nails was observed (Fig 1d–g, Extended Data Fig. 3 and Supplementary Videos 4 and 5). Mycobacterium leprae DNA was detected in all samples from June 2018 (Extended Data Table 2, Supplementary Table 2 and Supplementary Note 2). Here, continuous noninvasive detection of M. leprae was associated with the onset and evolution of a leprosy-like disease.

Retrospective PCR screening of all chimpanzee spleen samples (n = 38 individuals) from the TNP necropsy collection led to the identification of M. leprae DNA in two further individuals. An adult female from the same community named Zora, who had been killed by a leopard in 2009, tested positive in both PCR assays. The presence of M. leprae DNA was confirmed by PCR in various other organs (Extended Data Table 2). Retrospective analyses of photographs taken in the years before her death showed progressive skin hypopigmentation and nodule development since 2007 (Extended Data Fig. 3). Formalin-fixed skin samples (hands and feet) were prepared for histopathological examination using haematoxylin and eosin as well as Fite-Faraco stains. The skin presented typical signs of lepromatous leprosy characterized by a diffuse cutaneous cell infiltration in the dermis and the subcutis clearly separated from the basal layer of the epidermis (Extended Data Fig. 4a). We detected moderate numbers of acid-fast bacilli (single or in clumps) within histiocytes, indicative of M. leprae (Extended Data Fig. 4b). As antibodies against the M. leprae-specific antigen phenolic glycolipid-I (PGL-I) are a hallmark of M. leprae infection in humans20, we also performed a PGL-I lateral flow rapid test21 on a blood sample from this individual, which showed strong seropositivity (Extended Data Fig. 4c). Faecal samples collected in the years before Zora’s death contained M. leprae DNA from 2002 onwards, implying at least 7 years of infection (Extended Data Table 2). In this case, disease manifestations, histopathological findings, serological and molecular data, as well as the overall course of the disease, all unambiguously point towards M. leprae-induced leprosy.

To ascertain whether other individuals in the south community of TNP were infected at the time of Zora’s death in 2009, cross-sectional screening of contact animals (n = 32) was performed by testing all available faecal samples (n = 176) collected in 2009 (Supplementary Table 2). Three other chimpanzees were PCR-positive in single samples, including Woodstock. Clinical symptoms of leprosy have not been observed in other individuals, despite daily monitoring of south community members for 20 years and of neighbouring communities for 40 years22,23. Considering that, over this period, 467 individuals have been observed, it seems that leprosy is a rare disease with low transmission levels in these chimpanzee communities.

To characterize the M. leprae strains causing leprosy in wild chimpanzees and to perform phylogenomic comparisons, we selected DNA extracts that were positive in both the RLEP and the less-sensitive 18-kDa PCR, which indicates relatively high levels of M. leprae DNA. For TNP, we selected individuals that were positive in multiple samples. Following targeted enrichment using hybridization capture, samples were subjected to Illumina sequencing. Sufficient M. leprae genome coverage was obtained for sample GB-CC064 (Guinea-Bissau) and for Zora (Côte d’Ivoire) with mean depth of 39.3× and 25.8×, respectively (Extended Data Table 2 and Supplementary Table 5). We generated 21 M. leprae genomes from human biopsies from five West African countries (Niger, Mali, Benin, Côte d’Ivoire and Senegal) and depth of coverage ranged from 4.7× to 170×. We assembled a dataset that included the genomes generated in this study and all previously available M. leprae genomes. Of the total 286 genomes, 64 originated from six West African countries (Extended Data Fig. 5 and Supplementary Note 5).

Bayesian and maximum-parsimony analyses (Extended Data Figs. 6 and 7) place the strain from Guinea-Bissau (GB-CC064) on branch 4, where it clusters outside the standard genotypes 4N, 4O and 4P, but within the so-called 4N/O genotype24,25 (Fig. 2a, c). This 4N/O genotype is rare and only comprises five M. leprae strains; one strain (Ng13-33) from a patient in Niger, two strains (2188-2007 and 2188-2014) obtained from a single patient in Brazil (of 34 strains in Brazil)26 and two strains from two captive nonhuman primates originating from West Africa (Ch4 and SM1)25. The branching order of these five strains and GB-CC064 was unresolved in our analyses, with a basal polytomy suggestive of star-like diversification within this genotype, and within the group comprising all genotype 4 strains (4N/O, 4N, 4P and 4O). Divergence from the most recent common ancestor for this group is estimated to have occurred in the sixth century ad (mean divergence time, 1,437 years ago, 95% highest posterior density (HPD) 1,132–1,736 years ago). The strain that infected Zora in Côte d’Ivoire, designated TNP-418, belongs to branch 2F, within which, the branching order was also mostly unresolved (Fig. 2a, b). The branch is currently composed of human strains from medieval Europe (n = 7) and modern Ethiopia (n = 2), and this genotype has thus far never been reported to our knowledge in West Africa. Bayesian analysis estimated a divergence time during the second century ad (mean of 1,873 years ago (95% HPD 1,564–2,204 years ago)), similar to previous predictions27.

a, Bayesian dated phylogenetic tree of 278 M. leprae genomes including the two new chimpanzee strains (in bold red). Hypermutated samples with mutations in the nth gene were excluded from the analysis. The tree is drawn to scale, with branch lengths representing years of age. Median estimates of node ages are shown in black above branches; 95% HPD intervals are shown in grey. Some M. leprae branches are collapsed to increase readability. b, Maximum parsimony tree of branch 2F. c, Maximum parsimony tree of the branch 4. The tree was initially constructed using 286 genomes (Supplementary Table 6), including 2 new chimpanzee strains (in bold red) and 21 new genomes from West Africa (in bold), 500 bootstrap replicates and M. lepromatosis as outgroup. Sites with missing data were partially deleted (80% genome coverage cutoff), resulting in 4,470 variable sites used for the tree calculation. Subtrees corresponding to branches were retrieved in MEGA765. Corresponding genotypes are indicated on the side of each subtree. Samples are binned according to geographical origin as given in the legend. Scale bars (b, c), number of nucleotide substitutions. Animal silhouettes are available under Public Domain licence at PhyloPic (http://PhyloPic.org/).

Full size image

Samples from Woodstock did not yield enough Illumina reads to reconstruct full genomes for phylogenomic analysis. However, single-nucleotide polymorphisms (SNPs) recovered from the few available Illumina reads and Sanger sequences derived from PCR products allowed us to assign this second M. leprae strain from Côte d’Ivoire to the same genotype as TNP-418 (Supplementary Note 5). Overall, phylogenomic analyses show that M. leprae strains in chimpanzee populations at CNP and TNP are not closely related.

The finding of M. leprae-induced leprosy in wild chimpanzee populations raises the question of the origin(s) of these infections. Mycobacterium leprae is considered a human-adapted pathogen and previous cases of leprosy affecting wildlife were compatible with anthroponosis. Therefore, the prime hypothesis would be human-to-chimpanzee transmission. Potential routes of transmission include direct (such as skin-to-skin) contact and inhalation of respiratory droplets and/or fomites, with the assumption that, in all cases, prolonged and/or repeated exposure is required for transmission11. Chimpanzees at CNP are not habituated to humans and are not approached at distances that would allow for transmission via respiratory droplets. Although these chimpanzees inhabit an agroforest landscape and share access to natural and cultivated resources with humans28, present-day human–chimpanzee direct contact is uncommon. The exact nature of historic human–chimpanzee interactions at CNP remains, however, unknown. For example, robust data on whether chimpanzees were kept as ‘pets’ or were hunted for meat are lacking. Long-term human–chimpanzee coexistence in this shared landscape makes humans the most probable source of chimpanzee infection. However, multiple individuals from several chimpanzee communities across CNP show symptomatic leprosy demonstrating that M. leprae is now probably transmitted between individuals within this population.

At TNP, the south chimpanzee community is distant from human settlements and agriculture. Human-to-animal transmission of pathogens has been shown at TNP29,30 but involved respiratory pathogens (pneumoviruses and human coronavirus OC43) that transmit easily and do not require prolonged exposure. In addition, M. leprae is thought to be transmitted from symptomatic humans31 and no cases of leprosy have been reported among researchers or local research assistants. Although a human source is impossible to rule out, low human contact coupled with the rarity of the M. leprae genotype detected in TNP chimpanzees among human populations in West Africa suggests that recent human-to-chimpanzee transmission is unlikely. This is supported by the absence of drug-resistant mutations (Supplementary Note 6). The relatively old age of the lineage leading to the chimpanzee strain at TNP nevertheless raises the possibility of an ancient human-to-chimpanzee transmission. However, the human population density 1,500–2,000 years ago was probably even lower than it is currently, making this unlikely. If such an ancient transmission had occurred and the bacterium had persisted for a long time in chimpanzees, it should have spread more broadly as observed in M. leprae-infected squirrels and armadillos3,16,17. Therefore, an ancient human-to-chimpanzee transmission is not the most plausible mechanism to explain the presence of M. leprae in chimpanzees at TNP.

These findings may be better explained by the presence of a nonhuman leprosy reservoir. As chimpanzees hunt frequently, transmission may originate from their mammalian prey32. Nonhuman primates are the most hunted prey at TNP33 and are hunted at CNP (Supplementary Note 3). Chimpanzees also consume other mammalian prey such as ungulates. Notably, this scenario assumes that the animal host range of M. leprae is even broader than is currently known. Perhaps more intriguingly, an environmental source may be at the origin of chimpanzee infections. Other mycobacteria can survive in water, including M. ulcerans and other non-tuberculous mycobacteria34,35, and molecular investigations have reported that M. leprae can survive in soil36. Experimental data also show that M. leprae multiplies in amoebae37, arthropods38 and ticks39, which could contribute to the persistence of the bacteria in the environment. Testing these hypotheses will require thorough investigation of the distribution of M. leprae in wildlife and the environment and so shed light on the overall transmission pathways of the pathogen.


Study sites

Observational study and sample collections were performed at CNP in southern Guinea-Bissau and TNP in western Côte d’Ivoire (Extended Data Fig. 1a). CNP (1,067 km2) comprises the Cubucaré peninsula in the sector of Bedanda, with the northeast of the park bordering the Republic of Guinea. The landscape at CNP consists of a mosaic of mainly mangroves, subhumid forest patches, savannah grassland and woodland, remnant forest strips dominated by palm groves as well as agriculture40. There are approximately 200 villages and settlements within the borders of the park, with an estimated human population of 24,000 individuals who comprise several ethnic groups41. Chimpanzees are not hunted for consumption within CNP due to local cultural beliefs and taboos42 but are sometimes killed in retaliation for foraging on crops43,44. There is a minimum of 12 chimpanzee communities at CNP41, all unhabituated to researchers, with approximately 35–60 individuals per community45,46. Numerous other wildlife taxa inhabit CNP, including six other nonhuman primate species41,47.

The TNP (5,082 km2) consists of an evergreen lowland rainforest and is the largest remaining primary forest fragment in West Africa. It is home to a wide range of mammals that include 11 different nonhuman primate species48,49. There are no settlements or agricultural areas inside the National Park. As of March 2021, the three habituated communities, north, south and east, comprised 22, 37 and 32 individuals, respectively, although community sizes have varied over time. Systematic health monitoring of these communities has been ongoing since 200023.

Longitudinal observations and health monitoring

At CNP, camera traps (Bushnell Trophy Cam models 119774, 119877 and 119875) were deployed at 211 locations, including across different habitat types (forest, mangrove-forest edge and orchards) within the home range of 8 of the 12 putative chimpanzee communities (Supplementary Table 1). Camera traps were set up over six data collection periods from 2015 to 2019 (Extended Data Table 1). Targeted camera traps were deployed to record and monitor chimpanzee behaviour and disease occurrence. To maximize the chances of recording specific behaviours and to identify leprosy-like symptoms in individuals, targeted camera traps were set up in locations that chimpanzees were known to use most often, sometimes in clusters, precluding uniform survey designs. Targeted camera traps were set up in video mode and were active 24 h per day. When triggered, targeted cameras recorded 10 to 60 s of video with a minimum interval of 0.6 s or 2 s, depending on the camera trap model. Furthermore, systematically placed camera traps were used to obtain measures of wildlife occurrence and habitat use across the heterogeneous landscape41. Systematic camera traps were deployed across central CNP, at a minimum distance of 1 km between sampling points, as well as within the home range of one chimpanzee community (Caiquene-Cadique) and were spaced at least 500 m from one another. The camera traps pointed towards animal paths (often chimpanzee paths), small human paths also used by wildlife and other areas presenting signs of animal activity. Systematic camera traps were set up to record three consecutive photographs when triggered. The GPS coordinates, habitat type, date, time and site description were recorded when setting up individual camera traps (targeted and systematic). Opportunistic observations of chimpanzees at CNP were made in 2013, during which chimpanzees were photographed and/or filmed using digital cameras.

Chimpanzees at TNP are fully habituated to human observers and all individuals in the habituated communities are individually identified. Behavioural and health monitoring of chimpanzees at TNP involves daily observation of habituated individuals by an interdisciplinary team comprising primatologists and veterinarians; investigations of wildlife mortality causes through necropsies on all animal carcasses found in the research area; and the collection of noninvasive samples such as faecal samples, laboratory investigations and the communication of the results to the park management for corrective and preventive measures22. Abnormalities in behaviour or clinical signs of disease are immediately reported and followed by detailed observation by the on-site veterinarian. To reduce the risk of transmission of human diseases to the chimpanzees, stringent hygiene measures have been put in place, including an initial 5-day quarantine for observers, keeping a distance of at least 7 m and obligatory wearing of masks, with only healthy observers allowed to work in the forest50,51.

Faecal and necropsy sample collection

At CNP, chimpanzee faecal samples were collected between July 2017 and December 2018. The date and putative chimpanzee community were recorded for each faecal sample. As defecation was rarely observed and to prevent the collection of redundant samples from the same individual, we avoided multiple samples found under the same chimpanzee nest and paid special attention if multiple samples were found in proximity on trails45,52,53. All samples were collected with the aid of a wooden spatula and stored at ambient temperature in 15-ml tubes containing NAP buffer54. All samples were sent to the Robert Koch Institute for laboratory analysis. Even though chimpanzee faeces are easily distinguishable from those of other species and were found in areas where chimpanzees had recently been present with associated signs such as feeding remains or knuckle prints, we genetically confirmed the presence of chimpanzee DNA in faecal samples that tested positive in either of the M. leprae PCRs or the mammal PCR for diet analysis (Supplementary Note 3).

At TNP, the long-term health monitoring programme includes continuous collection of faecal and urine samples from known adult chimpanzees. Faeces are collected right after defecation, transferred to 2-ml cryotubes with the aid of a plastic spatula and frozen in liquid nitrogen the same day. A full necropsy is systematically performed on chimpanzees found dead by the on-site veterinarian. Necropsies follow a standardized biosafety protocol due to the occurrence of anthrax, Ebola and monkeypox in the area. This includes the use of full personal protective equipment and rigorous disinfection measures. Tissue samples of several internal organs are taken if the state of carcass decomposition allows. After collection, all samples are first stored in liquid nitrogen and subsequently shipped on dry ice to the Robert Koch Institute for analyses.

DNA extraction from faeces and necropsy samples

DNA extractions were performed at the Robert Koch Institute in a laboratory that has never been used for molecular M. leprae investigations. DNA was extracted from faecal and necropsy samples using the GeneMATRIX stool DNA purification kit (EURx) and the DNeasy Blood and Tissue kit (QIAGEN), respectively, following the manufacturers’ instructions. Extracted DNA was then quantified using the Qubit dsDNA HS Assay kit (Thermo Fisher Scientific) and subsequently stored at −20 °C until further use.

Genetic identification of samples from infected chimpanzees at CNP

To determine whether faecal samples positive for M. leprae belonged to one or two individuals at CNP, we amplified chimpanzee DNA at 11 microsatellite loci and one sexing marker55. Owing to the small quantity of starting DNA, not all loci were amplified and in some cases the amplification quality was low, affecting our ability to confidently interpret allele peak profiles (for example, sample GB-CC064 failed to amplify for 5 out of the 11 loci) (Supplementary Note 4).

Molecular screening of M. leprae in faecal and necropsy samples

Mycobacterium leprae DNA was searched for using two nested PCR systems targeting the distinct but conserved repetitive element RLEP and the 18-kDa antigen gene as previously described (Extended Data Table 3). As 37 copies of RLEP are present in the M. leprae genome, this assay is considered to be more sensitive than 18 kDa, for which there is only a single copy. To prevent contamination at the laboratory at the Robert Koch Institute and to enable us to identify whether it occurs, we followed these procedures: (1) separate rooms were used for preparation of PCR master mixes and the addition of DNA in the primary PCR; (2) the addition of the primary PCR product in the nested PCR in another separate room; and (3) dUTPs were used for all PCRs instead of dNTPs. For both assays, primary PCRs were performed in 20-µl reactions: up to 200 ng of DNA was amplified using 1.25 U of high-fidelity Platinum Taq polymerase (Thermo Fisher Scientific), 10× PCR buffer, 200 µM dUTPs, 4 mM MgCl2 and 200 nM of both forward and reverse primers. The thermal cycling conditions for the primary and nested PCRs were as follows: denaturation at 95 °C for 3 min, followed by 50 cycles of 95 °C for 30 s, 55 °C (18 kDa primers) or 58 °C (RLEP primers) for 30 s, and 72 °C for 1 min as well as an elongation step at 72 °C for 10 min. For nested PCRs, 2 µl of a 1:20 dilution of the primary PCR product was used as a template. Molecular-grade water was used as a template-free control. PCR products were visualized on a 1.5% agarose gel stained with GelRed (Biotium). Bands of the expected size were purified using the Purelink Gel extraction kit (Thermo Fisher Scientific). Both RLEP and 18-kDa nested PCR products are too short for direct Sanger sequencing. Therefore, fusion primers (primary PCR primers coupled with M13F and M13R primers) (Extended Data Table 3) were used for further amplification of the cleaned PCR products, applying the same conditions as in the primary PCR, but running only for 25 cycles. The resulting extended PCR products were then enzymatically cleaned using the ExoSAP-IT PCR Product Cleanup assay (Thermo Fisher Scientific) and Sanger sequenced using M13 primers. Resulting sequences were compared to publicly available nucleotide sequences using the Basic Local Alignment Search Tool (BLAST)56.


To further confirm the infection, skin samples were sent to the German Primate Center in Göttingen, Germany for histopathological analyses. Samples were immersion-fixed in 10% neutral-buffered formalin, embedded in paraffin and stained with standard haematoxylin and eosin using the Varistain Gemini staining automat (Thermo Fisher Scientific). Samples were also stained with Fite-Faraco stain for the identification of acid-fast bacilli.


A whole-blood sample from Zora collected during the necropsy in 2009 was tested for the presence of the M. leprae-specific anti-PGL-I antibodies using a chromatographic immunoassay developed for use with human blood following the instructions provided by the test manufacturers with a 1:10 diluted whole-blood sample. This rapid lateral flow test was produced by R. Cho using the synthetic ND-O-BSA antigen with financial support of the NIH/NIAID Leprosy Research Materials contract AI-55262 at Colorado State University. Test results were interpreted at 5 and 10 min. Human serum from a patient with multibacillary leprosy donated by J. S. Spencer, Colorado State University, was used as a positive control. Whole blood collected during the necropsy of a chimpanzee (Olivia) at TNP who died of acute respiratory disease in 2009 was used as a negative control.

Library preparation, genome-wide capture and high-throughput sequencing for nonhuman primate samples

Selected M. leprae-positive faecal and necropsy samples (Supplementary Table 2) were converted into dual-indexed libraries using the NEBNext Ultra II DNA Library Prep kit (New England Biolabs)57,58. To reconstruct whole genomes, libraries were target-enriched for M. leprae DNA using in-solution hybridization capture with 80-nt RNA baits designed to cover the whole M. leprae genome (twofold tiling; design can be shared upon request to the corresponding author) and following the myBaits protocol as previously described25. Around 1.5 µg of each DNA library was captured in single or pooled reactions. Two rounds of 24-h hybridization capture were performed followed by a post-amplification step for each using the KAPA HiFi HotStart Library Amplification kit with 12 to 16 cycles to generate around 200 ng of enriched library per sample. Finally, enriched libraries were purified using the silica-based MinElute reaction cleanup kit (QIAGEN) followed by quantification with the KAPA library quantification kit (Roche). Libraries were then normalized and pooled across sequencing lanes on an Illumina NextSeq 500 for sequencing with a mid-output kit v.2 for 300 cycles (Illumina).

Sample collection, DNA extraction, library preparation, genome-wide capture and high-throughput sequencing of human specimens

Samples (skin biopsies or DNA extracts) from patients with leprosy from five West African countries who had a positive bacillary index (Niger (n = 5), Mali (n = 8), Benin (n = 6), Côte d’Ivoire (n = 1) and Senegal (n = 1)) were obtained from the respective National Leprosy Control Programmes in the framework of the leprosy drug-resistance surveillance programmes or from previous investigation59.

DNA was extracted from skin biopsies using the total DNA extraction method as described previously60. DNA was quantified with a Qubit fluorometer using the Qubit dsDNA BR Assay kit (Thermo Fisher Scientific) before library preparation. DNA libraries were prepared using the KAPA Hyper Prep kit (Roche) as per the manufacturer’s recommendation using KAPA Dual-Indexed Adapter (Roche) followed by in-solution capture enrichment with 80-nt RNA baits with 2× tiling density for 48 h at 65 °C as described previously60. Post-capture amplification was performed with seven cycles. Enriched libraries were purified using a 1× ratio of KAPA Pure beads (Roche) followed by quantification with the KAPA library quantification kit (Roche) and quality control of the fragment with the Agilent 2200 TapeStation (Agilent Technologies). Libraries were then normalized and pooled across sequencing lanes on an Illumina NextSeq 500 for sequencing with a high output kit v.2 for 75 cycles (Illumina).

Genomic data analysis

Raw reads were processed as described elsewhere24. Putative unique variants of GB-CC064 and TNP-418 strains were manually checked and visualized using the Integrative Genomics Viewer61.

Genome-wide comparison and phylogenetic tree

SNPs of the two newly sequenced genomes from chimpanzees were compared to the 263 publicly available M. leprae genomes25,60,62,63,64 (Supplementary Table 6) and 21 new genomes from West African countries (Supplementary Note 5). Phylogenetic analyses were performed using a concatenated SNP alignment (Supplementary Table 7). Maximum-parsimony trees were constructed in MEGA765 with the 286 genomes available (Supplementary Table 5) using 500 bootstrap replicates and M. lepromatosis66 as outgroup. Sites with missing data were partially deleted (80% genome coverage cutoff), resulting in 4,470 variable sites used for the tree calculation.

Dating analysis

Dating analyses were performed using BEAST2 (v.2.5.2)67 as described previously24 with 278 genomes and an increased chain length from 50 to 100 million. In brief, concatenated SNPs for each sample were used for tip dating analysis (Supplementary Table 7). Hypermutated strains and highly mutated genes associated with drug resistance (in yellow, Supplementary Table 7) were omitted24,60, manual curation of the maximum parsimony and BEAST input file was conducted at the positions described in Supplementary Table 9 for GB-CC064 and TNP-418. Sites with missing data as well as constant sites were included in the analysis, as previously described24. Only unambiguous constant sites (loci where the reference base was called in all samples) were included.

PCR genotyping of insufficiently covered M. leprae genomes from positive chimpanzees

The genome coverage for the strain infecting Woodstock was low. To be able to determine the genotype, we identified specific variants from the genome-wide comparison of TNP-418 (the strain infecting Zora, an individual from the same social group) with other strains from branch 2F (Supplementary Table 9). Variants were manually checked and visualized in the partially covered genome from the strain infecting Woodstock using IGV software (Supplementary Table 10). Two variants not covered by high-throughput sequencing data were also selected for specific PCR screening. Primers were designed using the Primer3 web tool (http://bioinfo.ut.ee/primer3-0.4.0/) based on Mycobrowser sequences68 and are described in Extended Data Table 3. All PCR conditions were the same as in the M. leprae screening PCRs except for the primer sets and associated annealing temperatures.

Ethical oversight

For chimpanzees, all data were collected in accordance with Best Practice Disease and Monitoring Guidelines developed by the Section on Great Apes, IUCN SSC Primate Specialist Group (IUCN SSC PSG SGA). The collection of samples was noninvasive. All proposed data collection and analyses adhered strictly to ethics guidelines of the Association for the Study of Animal Behaviour (UK). Ethical approval for targeted leprosy camera trap surveys and faecal sample collection at CNP, Guinea-Bissau, was granted by the University of Exeter, UK. The Institute for Biodiversity and Protected Areas in Guinea-Bissau approved and collaborated directly on all aspects of this research. Ethical approval for the work by the Taï Chimpanzee Project at TNP was given by the Ethics Commission of the Max Planck Society. The Centre Suisse de Recherches Scientifiques en Côte d’Ivoire collaborates on the research at TNP.

For human participants, this study was carried out under the ethical consent of the World Health Organization Global Leprosy Program surveillance network. All human participants gave written informed consent in accordance with the Declaration of Helsinki.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this paper.

Data availability

Sequence data are available from the National Center for Biotechnology Information Sequence Read Archive, BioProject (PRJNA664360) and BioSample (16207289–16207321). BioSample codes for all samples used in this study are given in the Supplementary Data. Other relevant data are available in the Article and its Supplementary Information.


  1. 1.

    Walker, S. L. et al. in Manson’s Tropical Infectious Diseases 23rd edn, 506–518 (Elsevier, 2014).

  2. 2.

    Truman, R. Leprosy in wild armadillos. Lepr. Rev.76, 198–208 (2005).

    PubMedArticlePubMed Central Google Scholar

  3. 3.

    Avanzi, C. et al. Red squirrels in the British Isles are infected with leprosy bacilli. Science354, 744–747 (2016).

    ADSCASPubMedArticlePubMed Central Google Scholar

  4. 4.

    Suzuki, K., Tanigawa, K., Kawashima, A., Miyamura, T. & Ishii, N. Chimpanzees used for medical research shed light on the pathoetiology of leprosy. Future Microbiol.6, 1151–1157 (2011).

    PubMedArticlePubMed Central Google Scholar

  5. 5.

    Meyers, W. M. et al. Leprosy in a mangabey monkey–naturally acquired infection. Int. J. Lepr. Mycobact. Other Mycobact. Dis.53, 1–14 (1985).

    CAS Google Scholar

  6. 6.

    Gormus, B. J. et al. A second sooty mangabey monkey with naturally acquired leprosy: first reported possible monkey-to-monkey transmission. Int. J. Lepr. Mycobact. Other Mycobact. Dis.56, 61–65 (1988).

    CAS Google Scholar

  7. 7.

    Valverde, C. R., Canfield, D., Tarara, R., Esteves, M. I. & Gormus, B. J. Spontaneous leprosy in a wild-caught cynomolgus macaque. Int. J. Lepr. Mycobact. Other Mycobact. Dis.66, 140–148 (1998).

    CAS Google Scholar

  8. 8.

    Han, X. Y. et al. A new Mycobacterium species causing diffuse lepromatous leprosy. Am. J. Clin. Pathol.130, 856–864 (2008).

    CASPubMedArticlePubMed Central Google Scholar

  9. 9.

    Han, X. Y. et al. Comparative sequence analysis of Mycobacterium leprae and the new leprosy-causing Mycobacterium lepromatosis. J. Bacteriol.191, 6067–6074 (2009).

    CASPubMedPubMed CentralArticle Google Scholar

  10. 10.

    Ridley, D. S. & Jopling, W. H. Classification of leprosy according to immunity. A five-group system. Int. J. Lepr. Mycobact. Other Mycobact. Dis.34, 255–273 (1966).

    CAS Google Scholar

  11. 11.

    Britton, W. J. & Lockwood, D. N. Leprosy. Lancet363, 1209–1219 (2004).

    PubMedArticlePubMed Central Google Scholar

  12. 12.

    World Health Organization. Leprosy (Hansen’s disease). https://www.who.int/westernpacific/healthtopics/leprosy (2020).

  13. 13.

    Araujo, S., Freitas, L. O., Goulart, L. R. & Goulart, I. M. B. Molecular evidence for the aerial route of infection of Mycobacterium leprae and the role of asymptomatic carriers in the persistence of leprosy. Clin. Infect. Dis.63, 1412–1420 (2016).

    PubMedArticlePubMed Central Google Scholar

  14. 14.

    Lastória, J. C. & Morgado de Abreu, M. A. M. Leprosy: review of the epidemiological, clinical, and etiopathogenic aspects - part 1. An. Bras. Dermatol.89, 205–218 (2014).

    PubMedPubMed CentralArticle Google Scholar

  15. 15.

    Monot, M. et al. On the origin of leprosy. Science308, 1040–1042 (2005).

    ADSCASPubMedArticlePubMed Central Google Scholar

  16. 16.

    Truman, R. W. et al. Probable zoonotic leprosy in the southern United States. N. Engl. J. Med.364, 1626–1633 (2011).

    CASPubMedPubMed CentralArticle Google Scholar

  17. 17.

    Sharma, R. et al. Zoonotic leprosy in the southeastern United States. Emerg. Infect. Dis.21, 2127–2134 (2015).

    CASPubMedPubMed Central Google Scholar

  18. 18.

    da Silva, M. B. et al. Evidence of zoonotic leprosy in Pará, Brazilian Amazon, and risks associated with human contact or consumption of armadillos. PLoS Negl. Trop. Dis.12, e0006532 (2018).

    MathSciNetPubMedPubMed CentralArticleCAS Google Scholar

  19. 19.

    Donoghue, H. D., Holton, J. & Spigelman, M. PCR primers that can detect low levels of Mycobacterium leprae DNA. J. Med. Microbiol.50, 177–182 (2001).

    CASPubMedArticlePubMed Central Google Scholar

  20. 20.

    Stefani, M. M. et al. Assessment of anti-PGL-I as a prognostic marker of leprosy reaction. Int. J. Lepr. Mycobact. Other Mycobact. Dis.66, 356–364 (1998).

    CAS Google Scholar

  21. 21.

    Spencer, J. S. & Brennan, P. J. The role of Mycobacterium leprae phenolic glycolipid-I (PGL-I) in serodiagnosis and in the pathogenesis of leprosy. Lepr. Rev.82, 344–357 (2011).

    PubMedArticlePubMed Central Google Scholar

  22. 22.

    Leendertz, F. H. et al. Pathogens as drivers of population declines: the importance of systematic monitoring in great apes and other threatened mammals. Biol. Conserv.131, 325–337 (2006).

    Article Google Scholar

  23. 23.

    Crockford, C., Vigilant, L., Deschner, T., & Leendertz, F. The Chimpanzees of the Taï Forest: 40 Years of Research (Cambridge Univ. Press, 2019).

  24. 24.

    Benjak, A. et al. Phylogenomics and antimicrobial resistance of the leprosy bacillus Mycobacterium leprae. Nat. Commun.9, 352 (2018).

    ADSPubMedPubMed CentralArticleCAS Google Scholar

  25. 25.

    Honap, T. P. et al. Mycobacterium leprae genomes from naturally infected nonhuman primates. PLoS Negl. Trop. Dis.12, e0006190 (2018).

    PubMedPubMed CentralArticleCAS Google Scholar

  26. 26.

    Stefani, M. M. A. et al. Whole-genome sequencing distinguishes between relapse and reinfection in recurrent leprosy cases. PLoS Negl. Trop. Dis.11, e0005598 (2017).

    PubMedPubMed CentralArticleCAS Google Scholar

  27. 27.

    Schuenemann, V. J. et al. Ancient genomes reveal a high diversity of Mycobacterium leprae in medieval Europe. PLoS Pathog.14, e1006997 (2018).

    PubMedPubMed CentralArticleCAS Google Scholar

  28. 28.

    Hockings, K. J., Parathian, H., Bessa, J. & Frazão-Moreira, A. Extensive overlap in the selection of wild fruits by chimpanzees and humans: implications for the management of complex social-ecological systems. Front. Ecol. Evol.8, 123 (2020).

    Article Google Scholar

  29. 29.

    Köndgen, S. et al. Pandemic human viruses cause decline of endangered great apes. Curr. Biol.18, 260–264 (2008).

    PubMedArticleCASPubMed Central Google Scholar

  30. 30.

    Patrono, L. V. et al. Human coronavirus OC43 outbreak in wild chimpanzees, Côte d’Ivoire, 2016. Emerg. Microbes Infect.7, 118 (2018).

    PubMedPubMed CentralArticle Google Scholar

  31. 31.

    Richardus, J. H., Ignotti, E. & Smith, W. C. S. in International Textbook of Leprosy (eds Scollard, D. M. & Gillis, T. P.) (2016).

  32. 32.

    Gogarten, J. F. et al. The ecology of primate retroviruses – an assessment of 12 years of retroviral studies in the Taï National Park area, Côte d’Ivoire. Virology460, 147–153 (2014).

    PubMedArticleCASPubMed Central Google Scholar

  33. 33.

    Boesch, C. & Boesch, H. Hunting behavior of wild chimpanzees in the Taï National Park. Am. J. Phys. Anthropol.78, 547–573 (1989).

    CASPubMedArticlePubMed Central Google Scholar

  34. 34.

    Stinear, T. et al. Identification of Mycobacterium ulcerans in the environment from regions in Southeast Australia in which it is endemic with sequence capture-PCR. Appl. Environ. Microbiol.66, 3206–3213 (2000).

    ADSCASPubMedPubMed CentralArticle Google Scholar

  35. 35.

    Rabinowitz, P. & Conti, L. Human-Animal Medicine: Clinical Approaches to Zoonoses, Toxicants and other Shared Health Risks (Elsevier, 2010).

  36. 36.

    Lahiri, R. & Adams, L. B. in International Textbook of Leprosy (eds. Scollard, D. M. & Gillis, T. P.) (2016).

  37. 37.

    Wheat, W. H. et al. Long-term survival and virulence of Mycobacterium leprae in amoebal cysts. PLoS Negl. Trop. Dis.8, e3405 (2014).

    PubMedPubMed CentralArticle Google Scholar

  38. 38.

    Neumann, A. et al. Experimental infection of Rhodnius prolixus (Hemiptera, Triatominae) with Mycobacterium leprae indicates potential for leprosy transmission. PLoS ONE11, e0156037 (2016).

    PubMed CentralArticleCAS Google Scholar

  39. 39.

    Ferreira, J. D. S. et al. Ticks as potential vectors of Mycobacterium leprae: use of tick cell lines to culture the bacilli and generate transgenic strains. PLoS Negl.Trop. Dis.12, e0007001 (2018).

    PubMedPubMed CentralArticleCAS Google Scholar

  40. 40.

    Catarino, L. M., Martins, E. S., Pinto-Basto, M. F. & Diniz, M. A. Plantas Vasculares e Briófitos da Guiné-Bissau (Instituto de Investigação Cientifica Tropical, 2006).

  41. 41.

    Bersacola, E., Hill, C. M. & Hockings, K. J. Chimpanzees balance resources and risk in an anthropogenic landscape of fear. Sci Rep.11, 4569 (2021).

    ADSCASPubMedPubMed CentralArticle Google Scholar

  42. 42.

    Parathian, H. E., McLennan, M. R., Hill, C. M., Frazão-Moreira, A. & Hockings, K. J. Breaking through disciplinary barriers: human–wildlife interactions and multispecies ethnography. Int. J. Primatol.39, 749–775 (2018).

    PubMedPubMed CentralArticle Google Scholar

  43. 43.

    Sousa, C. & Frazão-Moreira, A. in Etnoecologia em Perspectiva: Natureza, Cultura e Conservação (eds Alves, A. G. C et al.) 187–200 (NUPEEA, 2010).

  44. 44.

    Sousa, J., Vicente, L., Gippoliti, S., Casanova, C. & Sousa, C. Local knowledge and perceptions of chimpanzees in Cantanhez National Park, Guinea-Bissau. Am. J. Primatol.76, 122–134 (2014).

    PubMedArticlePubMed Central Google Scholar

  45. 45.

    Bessa, J., Sousa, C. & Hockings, K. J. Feeding ecology of chimpanzees (Pan troglodytes verus) inhabiting a forest-mangrove-savanna-agricultural matrix at Caiquene-Cadique, Cantanhez National Park, Guinea-Bissau. Am. J. Primatol.77, 651–665 (2015).

    PubMedArticlePubMed Central Google Scholar

  46. 46.

    Vieira, W. F., Kerry, C. & Hockings, K. J. A comparison of methods to determine chimpanzee home-range size in a forest–farm mosaic at Madina in Cantanhez National Park, Guinea-Bissau. Primates60, 355–365 (2019).

    PubMedPubMed CentralArticle Google Scholar

  47. 47.

    Hockings, K. J. & Sousa, C. Human–chimpanzee sympatry and interactions in Cantanhez National Park, Guinea-Bissau: current research and future directions. Primate Conserv.26, 57–65 (2013).

    Article Google Scholar

  48. 48.

    McGraw, S., Zuberbühler, K. & Noë, R. Monkeys of the Taï Forest: An African Primate Community (Cambridge Univ. Press, 2007).

  49. 49.

    Boesch, C. & Boesch-Achermann, H. The Chimpanzees of the Taï Forest: Behavioural Ecology and Evolution (Oxford Univ. Press, 2000).

  50. 50.

    Gilardi, K. V. K. et al. Best Practice Guidelines for Health Monitoring and Disease Control in Great Ape Populations (IUCN, 2015).

  51. 51.

    Grützmacher, K. et al. Human quarantine: toward reducing infectious pressure on chimpanzees at the Taï Chimpanzee Project, Côte d’Ivoire. Am. J. Primatol.80, e22619 (2018).

    Article Google Scholar

  52. 52.

    McLennan, M. R. Diet and feeding ecology of chimpanzees (Pan troglodytes) in Bulindi, Uganda: foraging strategies at the forest–farm interface. Int. J. Primatol.34, 585–614 (2013).

    Article Google Scholar

  53. 53.

    McCarthy, M. S. et al. Genetic censusing identifies an unexpectedly sizeable population of an endangered large mammal in a fragmented forest landscape. BMC Ecol.15, 21 (2015).

    PubMedPubMed CentralArticleCAS Google Scholar

  54. 54.

    Camacho‐Sanchez, M., Burraco, P., Gomez‐Mestre, I. & Leonard, J. A. Preservation of RNA and DNA from mammal samples under field conditions. Mol. Ecol. Resour.13, 663–673 (2013).

    PubMedArticleCASPubMed Central Google Scholar

  55. 55.

    Borges, F. F. A Country-level Genetic Survey of the IUCN Critically Endangered Western Chimpanzee (Pan troglodytes verus) in Guinea-Bissau (Univ. Porto, 2017).

  56. 56.

    Altschul, S. F., Gish, W., Miller, W., Myers, E. W. & Lipman, D. J. Basic local alignment search tool. J. Mol. Biol.215, 403–410 (1990).

    CASPubMedPubMed CentralArticle Google Scholar

  57. 57.

    Mubemba, B. et al. Yaws disease caused by Treponema pallidum subspecies pertenue in wild chimpanzee, Guinea, 2019. Infect. Dis. J.26, 1283–1286 (2020).

    Google Scholar

  58. 58.

    Patrono, L. V. et al. Monkeypox virus emergence in wild chimpanzees reveals distinct clinical outcomes and viral diversity. Nat. Microbiol.5, 955–965 (2020).

    PubMedArticleCASPubMed Central Google Scholar

  59. 59.

    Monot, M. et al. Comparative genomic and phylogeographic analysis of Mycobacterium leprae. Nat. Genet.41, 1282–1289 (2009).


Sours: https://www.nature.com/articles/s41586-021-03968-4

Eyebrow Contouring with Hyaluronic Acid Gel Filler Injections

J Clin Aesthet Dermatol. 2018 Feb; 11(2): 38–40.

Published online 2018 Feb 1.

Author informationCopyright and License informationDisclaimer

Dr. Mustak is with the University of Cape Town Groote Schuur Hospital in Cape Town, Western Cape, South Africa.

Drs. Mustak, Fiaschetti, Gupta, and Goldberg are with the Stein Eye Institute, University of California in Los Angeles, California.

corresponding authorCorresponding author.

CORRESPONDENCE: Hamzah Mustak, FCOphth(SA); Email: [email protected]

FUNDING:No funding was provided for this article.

DISCLOSURES:The authors have no conflicts of interest to relevant to the content of this article.

Copyright © 2018. Matrix Medical Communications. All rights reserved.


Background: The eyebrow region presents challenges for filling: the skin is thick, the three-dimensional anatomy is complex and there is a predisposition towards fat atrophy and skeletonization with aging. Hyaluronic acid gel fillers are well known for their use in the periorbital region. We report our long-term experience with eyebrow filling over a period of five years. Methods: Twenty cases of periorbital eyebrow filling with hyaluronic acid gel fillers were followed up over a period of five years. The eyebrow filling was customized based on the patient’s anatomical features in a three-dimensional plane. Standardized photographs before and after the procedure in standard lighting conditions were evaluated. Results: Hyaluronic acid gel fillers were tolerated well in the eyebrow region. There were no cases with blue-gray dyschromia or prolonged edema as is the case with lower eyelid injections. The eyebrow gained volume and looked fuller immediately after the injection. There were three cases with excessive eyebrow puffiness noted on a long-term follow-up which may be the accumulated filler weighing the eyebrow. No other adverse events were noted. Conclusion: The eyebrow anatomy is a complex three-dimensional structure. Deflation in the eyebrow area along with the superior sulcus occurs with aging. Filling the eyebrow with hyaluronic acid gel fillers is a useful tool in the armamentarium of the cosmetic facial surgeon and can be used in isolation in select patients or as an adjunct to surgical rehabilitation. We believe the fillers last longer and are well tolerated in the eyebrow region due to the complex anatomy specific to this region.

Keywords: Eyebrow, filler, facial rejuvenation

The eyelid-eyebrow unit plays an important role in facial aesthetics. The eyebrow is distinctive in its structure and forms the framework for the upper eyelid. In younger individuals, the eye looks longer and fuller with thicker, elastic skin. As we age, the skin loses elasticity, the tissues deflate, and the underlying bony orbital rim is exposed.1,2 In addition, the eyebrows simultaneously undergo characteristic aging changes. The brow position droops by a few millimeters, more laterally than medially, and the eyebrow fat pad shrinks, leading to a flatter appearance and loss of three-dimensional projection.13

Facial re-inflation has been practiced for centuries, with reports of paraffin being used in Greece in the early 19th century.4 Autologous fat injection, in combination with blepharoplasty and fillers, has been used with variable success in the peri-orbital region.57 Volume enhancement of the aging face, although not a substitute for conventional surgery, is a promising alternative.6,7,8 The concept of nonsurgical rejuvenation and tissue inflation rather than excision is gaining attention as our understanding of aging improves. There is a subset of patients who are poor candidates for surgical rejuvenation. For these patients, volume enhancement with hyaluronic acid gels is a promising treatment modality. When assessing the eyebrow unit aesthetically, it is important to differentiate the eyebrow hairs from the three-dimensional eyebrow shape. The geographic distribution of the eyebrow hairs can be altered by reduction (e.g., waxing, plucking, threading) or by augmentation (e.g., makeup, tattooing, microblading). The three-dimensional shape is very important in facial aesthetics and changes with aging; it can be improved with reduction (e.g., eyebrow fat debulking, orbital rim shaving) or augmentation (e.g., fat, synthetic fillers). In this retrospective chart review, we report our long-term experience with hyaluronic acid gels (HAG) as a treatment modality for adding volume to the three-dimensional eyebrow shape.


This retrospective study reviewed the charts of patients who were administered HAG. All the patients who had eyebrow filler injections within the past ten years with the following criteria were included: 1) minimum follow-up of five years; 2) no history of eyelid or eyebrow surgery within the follow-up duration; and 3) no history of neurological disease.

All the injections were performed by a single oculoplastic surgeon. Using the HAG Restylane-L (Galderma, Fort Worth, Texas), use of which was based on surgeon experience and preference. Injections were carried out under topical anesthesia that was applied 30 to 60 minutes before the procedure. Treatment area was sterilized with alcohol immediately before the injections. Using a 30-gauge needle, the HAG was applied in the retro-orbicularis oculi fat (ROOF) pad in the tissue plane deep to the orbicularis oculi muscle (Figure 1A–B). A feathering technique was employed using multiple passes of the needle to create a haystack configuration of multiple fine threads, layered and feathered to create the desired three-dimensional contour. Bruising is primarily associated with passage of the needle through the orbicularis layer. To minimize bruising, the needle is only withdrawn all the way out through the skin when repositioning is required or for another series of passages. Once the needle is deep to the orbicularis, the surgeon takes advantage of the sub-orbicularis plane by creating a fan-shaped pattern of passes without withdrawing the needle completely. If bruising or hematomas start to form, the area is treated with gentle pressure from a cotton tip applicator. If the needle is placed too superficially, visible lumps or wheals of the HAG will form. It is important, therefore, to avoid depositing large volumes of the filler in one location. Gentle, continuous pressure is applied to the syringe plunger as the needle is slowly fanned through the tissues to create smooth, feathered, three-dimensional contours. The shape is customized to the patient and the degree of volume, whether applied in the superior aspect of the eyebrow fat pad, the inferior aspect of the eyebrow fat pad, feathered laterally into the temporalis muscle fossa, or added along the deep orbital rim to fill the superior sulcus, will vary from patient to patient. A clinical effect with an appreciable change in eyebrow contour is visible during and immediately after the procedure.


The upper orbital space is a key three-dimensional contour defining periorbital aesthetics.10 In youth, fullness of the dermis, subcutaneous fat pads, and deep fat pads create a three-dimensional fullness that defines the aesthetics of the youthful eyelid.13 With aging, loss of volume in the dermis and various fat pads can create a sagging appearance, drawing inelastic skin into the eyelid space and creating the appearance of eyebrow drooping.11 In addition, there is likely some actual gravitational descent of the lateral eyebrow, but this is generally less important than deflation in creating the aged appearance.

Rehabilitation of the aging upper orbit is most effective when this loss of volume is taken into account. Conversely, rehabilitative paradigms that focus primarily on elevating the eyebrow are suboptimal in re-creating the contours of youth. The smooth, full, three-dimensional shape created by the subcutaneous and deep fat pads characterizes the eyebrow.12,13 This contour covers the orbital rim and extends variably into the eyelid space itself. By projecting the skin forward, the three dimensional volume essentially elevates the eyelid skin out of the orbital space in a similar way that a full balloon stretches and smoothes the rubber surface. We noted heavy eyebrows and puffiness in three patients; this could have been due to the filler substance accumulation over repeated injections.

There have been various recommendations about the position of injection. Lucarelli and colleagues14 demonstrated that injecting in the pre-periosteal plane requires less volume while achieving a robust result. Lambros15 recommends injecting into the sub-orbicularis and subcutaneous fat, while Glasgold16 recommends injecting into the subcutaneous plane. The ROOF extends from the eyebrow region that drapes over the superior orbital rim to the upper eyelid. This fat pad contributes to the smooth contour over the superior orbital rim. We find that injecting into the plane of the ROOF is effective in creating smooth, appropriate contours. Growing out of this three-dimensional structure of the eyebrow fat pad and three-dimensional shape are the eyebrow hairs. The thickness, geographic distribution, and shape of the eyebrow hair vary substantially. Certainly, the eyebrow hairs effect appearance and are the subject of a vast industry focused on shaping, coloring, thinning, removing or tattooing hairs to effect the geographic distribution. We suggest avoiding being distracted by the distribution of the eyebrow hairs when assessing the three-dimensional shape of the eyebrow.


We have had good success filling the eyebrow fat pad to change the three-dimensional shape of the eyebrow complex. The shape of the eyebrow fat pad, and its extensions into the superior orbital space and temporalis fossa, varies across individuals. HAG filler alone is particularly useful for patients who are poor candidates for surgery or want to avoid surgery. It might also be a useful tool in conjunction with surgery to address the volume depletion seen with aging.

The primary goal of eyebrow surgery or filling should be to improve the three-dimensional shape of the eyebrow complex, rather than focusing on the distribution of the eyebrow hairs. For optimal results, the distribution of filler should be customized to the patient in an artistic manner. In our anecdotal experience, subtle sculpting of the shape of the eyebrow complex with HAG fillers can help achieve acceptable cosmetic endpoints for eyebrow contouring.


1. Lambros V. Observations on periorbital and midface aging. Plast Reconstr Surg. 2007;120:1367–1376. [PubMed] [Google Scholar]

2. Lambros V. Models of facial aging and implications for treatment. Clin Plast Surg. 2008;35:319–327. [PubMed] [Google Scholar]

3. Shaw RB, Jr, Katzel EB, Koltz PF, et al. Aging of the facial skeleton: aesthetic implications and rejuvenation strategies. Plast Reconstr Surg. 2011;127:374–383. [PubMed] [Google Scholar]

4. Goldwyn RM. The paraffin story. Plast Reconstr Surg. 1980;65:517–522. [PubMed] [Google Scholar]

5. Lambros V. Fat injection for the aging midface. Oper Tech Plast Reconstr Surg. 1998;5:130–137.[Google Scholar]

6. Goldberg RA, Fiaschetti D. Filling the periorbital hollows with hyaluronic acid gel: initial experience with 244 injections. Ophthal Plast Reconstr Surg. 2006;22:335–341. [PubMed] [Google Scholar]

7. Hoenig J, Hoenig D. Minimally invasive periorbital rejuvenation. Facial Plast Surg. 2013 Aug;29(4):295–309. [PubMed] [Google Scholar]

8. Kornstein AN. Soft-tissue reconstruction of the brow with Restylane. Plast Reconstr Surg. 2005;116:2017–2020. [PubMed] [Google Scholar]

9. Rootman DB, Lin JL, Goldberg R. Does the Tyndall effect describe the blue hue periodically observed in subdermal hyaluronic acid gel placement? Ophthal Plast Reconstr Surg. 2014;30:524–527. [PubMed] [Google Scholar]

10. Gunter JP, Antrobus SD. Aesthetic analysis of the eyebrows. Plast Reconstr Surg. 1997;99(7):1808–1816. [PubMed] [Google Scholar]

11. Papageorgiou KI, Mancini R, Garneau HC, et al. A three-dimensional construct of the aging eyebrow: the illusion of volume loss. Aesthet Surg J. 2012;32:46–57. [PubMed] [Google Scholar]

12. Hwang SH, Hwang K, Jin S, et al. Location and nature of retro-orbicularis 141 oculus fat and suborbicularis oculi fat. J Craniofac Surg. 2007;18:387–390. [PubMed] [Google Scholar]

13. Charpy M. Le coussinex adipoeux du sourcil. Bibliog Anat. 1909;19:47–52.[Google Scholar]

14. Griepentrog GJ, Lucarelli MJ. Anatomical position of hyaluronic acid gel following injection to the eyebrow. Ophthal Plast Reconstr Surg. 2013;29:364–366. [PubMed] [Google Scholar]

15. Lambros V. Volumizing the brow with hyaluronic acid fillers. Aesthet Surg J. 2009;29:174–179. [PubMed] [Google Scholar]

16. Glasgold M, Lam SM, Glasgold R. Volumetric rejuvenation of the periorbital region. Facial Plast Surg. 2010 Aug;26(3):252–259. [PubMed] [Google Scholar]

Articles from The Journal of Clinical and Aesthetic Dermatology are provided here courtesy of Matrix Medical Communications

Sours: https://www.ncbi.nlm.nih.gov/pmc/articles/PMC5843360/
  1. Pastel brushes procreate
  2. Tocd feels real
  3. Pokemon go mod apk ios
  4. Gta 5 mods discord server

How to Find the Right Eyebrow Color for Your Hair

Choosing a new hair color is serious business. It's a journey that starts way before you sit down in your colorist's chair. Scrolling through Instagram for inspiration, creating a Pinterest board for each possible shade, and reading up on what colors work well with your skin tone are all crucial steps leading up to your salon appointment.

When you're so focused on switching up your hair color, it's easy to overlook your eyebrows, but it's equally important that the shade of your brows also compliments your new dye job.  

"Your hair on your face and around your face should frame and enhance your natural beauty," says Christine Thompson, co-owner and color director at Spoke & Weal. "Getting the tones and level right are essential to translating your look, whether it’s soft or strong." 

Amy Clark of Rob Peetoom Salon New York says to make sure the shade of your brows compliments the tones in your hair color. "My general rule would be to keep it as close to the shade of your hair as best as possible, or one shade darker," she says. Going too dark can look severe. 

And if you have virgin hair, but want to fill in your brows. This advice goes for makeup products, too. Daniel Chinchilla, celebrity makeup artist and owner of Chinchilla Brows recommends brow powder for a soft, natural look, and a pencil if you're going for definition. 

So, what color is right for you? Keep scrolling for a complete breakdown on the best eyebrow shade for your hair.

VIDEO: How to Use Tinted Brow Gel

Start Slideshow

Sours: https://www.instyle.com/hair/best-eyebrow-color-for-hair


Eyebrows 4c




You will also be interested:


406 407 408 409 410